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Pex13p degradation in yeastChen, Xin
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Pex13p degradation in yeast
PhD thesis
Xin Chen(陈新)
The studies presented in this thesis were performed in the research group Cell
Biochemistry of the Groningen Biomolecular Sciences and Biotechnology
Institute (GBB) of the University of Groningen, The Netherlands.
ISBN digital version: 978-94-034-1616-8
ISBN printed version: 978-94-034-1617-5
Cover design and layout: Chen Xin, Richard Mohler, Ilse Modder
Inner layout: Chen Xin, Ilse Modder, www.ilsemodder.nl
Printing: Gildeprint Enschede
© 2019 Chen Xin, Groningen, The Netherlands
All rights reserved.
Pex13p degradation in yeast
Phd thesis
to obtain the degree of PhD at the
University of Groningen
on the authority of the
Rector Magnificus prof. E. Sterken
and in accordance with
the decision by the College of Deans.
This thesis will be defended in public on
Friday 24 May 2019 at 11.00 hours
by
Xin Chen
born on 29 August 1987
in Neimongol, China
Supervisor
Prof. P.J.M. van Haastert
Co-supervisor
Dr. C.P. Williams
Assessment Committee
Prof. A.J.M. Driessen
Prof. S.J. Marrink
Prof. M. Schrader
Table of contents
Chapter 1 Introduction: From peroxisome formation to peroxisomal
membrane protein degradation
7
Aim and Outline 35
Chapter 2
Insights into the role of the peroxisomal ubiquitination
machinery in Pex13p degradation in the yeast Hansenula
polymorpha
39
Chapter 3
Further insights into Pex13p degradation in the yeast
Hansenula polymorpha
69
Chapter 4
Investigating Pex13p degradation in the yeast Saccharomyces
cerevisiae
105
Chapter 5
Insights into fungal peroxisome function gained from
organellar proteomics based approaches
143
References 160
Chapter 6 Summary and Discussion 189
Samenvatting 195
Acknowledgments 201
1
Chapter 1
Introduction: From peroxisome formation to peroxisomal membrane protein
degradation
Xin Chen and Chris Williams
ONE Introduction
8
1. Introduction
Eukaryotic cells separate a number of processes into distinct compartments. Such
compartments, known as organelles, allow for the creation of different environments
within a cell, which helps to increase the efficiency of these cellular processes and also
to allow them to be regulated separately from other parts of the cell. One such organelle
is the peroxisome (Gabaldon, 2010). Peroxisomes were first identified by electron
microscopy as small and single membrane-bound vesicles present in kidney tissue cells
(Rhodin, 1954). Later, biochemical approaches demonstrated that peroxisomes produce
hydrogen peroxide and contain enzymes that function in the production and degradation
of hydrogen peroxide, which led to them receiving the name “peroxisome” (De Duve &
Baudhuin, 1966; Rhodin, 1954). Since this time, the number of functions prescribed to
peroxisomes has increased dramatically and it is likely that additional functions remain
to be discovered.
Peroxisome function depends upon the organism and cell type under inspection.
Other than the decomposition of reactive oxygen species such as hydrogen peroxide,
peroxisomes in many organisms play a prominent role in fatty acid β-oxidation
(Bonekamp et al, 2009). In yeasts and plants, fatty acid β-oxidation takes place
exclusively in peroxisomes (Kindl, 1993; Kunau et al, 1988) while in mammals and
certain filamentous fungi, the β-oxidation of fatty acids is divided between the
mitochondria and peroxisomes (Kunau et al, 1988). In addition, peroxisomes in certain
organisms are involved in the catabolism of D-amino acids, polyamines and
biosynthesis of plasmalogens and certain antibiotics but many more peroxisomal
functions exist (Islinger et al, 2010). Such functional diversity has led to certain
peroxisome-like organelles being given different names, such as glyoxysomes
(containing enzymes of the glyoxylate cycle) in filamentous fungi such as Neurospora
crassa (Keller et al, 1991) and glycosomes (involved in glucose metabolism) in
members of the trypanosome family of parasites (Opperdoes, 1987).
The proteins that are responsible for peroxisome maintenance have been given the
name Peroxin (Gould & Valle, 2000). To date, 36 Peroxins (Pex for short) have been
identified and these proteins are encoded by PEX genes. Many Pex proteins are well
conserved throughout evolution (such as Pex5p and Pex3p) whereas a number can only
be found in certain organisms (such as Pex33p in N. crassa).
Loss of peroxisome function can have a detrimental effect on cell vitality. For
example, Hansenula polymorpha yeast cells that lack functional peroxisomes cannot
grow on media containing methanol, because methanol degradation occurs exclusively
inside peroxisomes (Baerends et al, 1996). Likewise, Arabidopsis thaliana seedlings
Introduction ONE
9
that display a peroxisome defect are inhibited in growth and suffer from developmental
delays (Woodward et al, 2014). In humans, peroxisomal defects are associated with a
range of different diseases known collectively as Zellweger spectrum disorders (ZSDs).
ZSDs include Zellweger syndrome, neonatal adreno-leukodystrophy and infantile
Refsum disease, listed from the most to the least severe (Waterham et al, 2016). ZSDs
show a wide range of symptoms which stem from an impairment in one or more
peroxisomal functions (Waterham & Ebberink, 2012). At the biochemical level, patients
suffering from ZSDs often display reduced levels of plasmalogens. These
ether-phospholipids, which are particularly essential for brain and lung function, are
synthesized in peroxisomes. In addition, ZSD patients also display elevated levels of
very long chain fatty acids (VLCFA) and branched chain fatty acids (BCFA) because
these fatty acids are degraded in peroxisomes. The accumulation of these fatty acids
compromises the function of multiple organs and can result in symptoms such as
enlarged liver, eye abnormalities, seizures; severe peroxisomal disorders can result in
premature death (Raymond et al, 2009; Steinberg et al, 2006).
The above-mentioned examples demonstrate how important peroxisome function is
for cell health. Hence, it is vital that peroxisome function is tightly regulated. Here we
present an overview of processes that regulate peroxisome function. We first describe
how peroxisomes form, outlining the possible mechanisms of peroxisome biogenesis,
followed by how peroxisomes are degraded by pexophagy. Next, we describe how
peroxisomal protein import is achieved, presenting the different mechanisms by which
peroxisomal membrane and matrix proteins target to peroxisomes. Furthermore, we
outline how the ubiquitin proteasome system, the major protein degradation pathway in
eukaryotic cells, regulates protein homeostasis. Finally, we introduce the topic of
peroxisomal proteomics and present our perspectives on several major questions that
remain to be answered in the peroxisome research field.
2. Peroxisome biogenesis
In general terms, organelles can be seen as either semi-autonomous (e.g. mitochondria,
chloroplasts (Boardman et al, 1971)) or as part of the endomembrane system (such as
the vacuole, endoplasmic reticulum (ER) and Golgi (Harris, 1986)). Organelles from the
endomembrane system import most of their proteins via the ER, often through vesicular
transport. Semi-autonomous organelles, on the other hand, either produce their own
proteins or import them directly from the cytosol. The processes governing peroxisome
formation, known as peroxisome biogenesis, seem to resemble biogenesis processes of
both semi-autonomous organelles (in that peroxisomes can multiply by fission, similar
ONE Introduction
10
to the mitochondria) and the endomembrane system (in that lipids and a set of
peroxisomal membrane proteins can traffic to peroxisomes via the ER). This has led to
two models for peroxisomal biogenesis being proposed; the de novo model and growth
and division model.
The de novo model (Fig. 1) suggests that peroxisomes form from vesicles derived
from the ER (reviewed in (Agrawal & Subramani, 2016)). Certain peroxisomal
membrane proteins (PMPs) target to the ER in yeast cells lacking Pex3p, a protein
involved in PMP import (Agrawal et al, 2011; Titorenko & Rachubinski, 1998; van der
Zand et al, 2010). pex3 cells were reported to lack peroxisome like structures
(Shimozawa et al, 2000). Upon reintroduction, Pex3p targets to the ER and initiates the
formation of peroxisomes at the ER. Other PMPs synthesized in the cytosol then target
to the ER membrane, where they are sorted into peroxisomal ER subdomains (pER)
which then bud off the ER in a Pex3p and Pex19p dependent manner. It was reported
that different vesicles bud from the ER, containing different PMPs required for either the
docking or the receptor recycling steps of peroxisomal matrix protein import (see
section on Protein import into peroxisomes). These heterotypic vesicles fuse in a
Pex1p/Pex6p dependent manner to form functional peroxisomes, which can then import
the matrix proteins (MATs) required for peroxisome function (Fakieh et al, 2013; van
der Zand et al, 2010; van der Zand et al, 2012). However, studies by other groups have
questioned whether such heterotypic vesicles exist (Knoops et al, 2015; Motley et al,
2015). Furthermore, recent studies in H. polymorpha pex3 cells propose an alternative
de novo model (Fig. 1). Knoops et al. demonstrated, contrary to previous reports
(Baerends et al, 1997), that pex3 cells possess tiny pre-peroxisomal vesicles (PPVs) that
contain a subset of PMPs. Upon reintroduction, Pex3p targets to these PPVs and
facilitates the import of other PMPs directly to PPVs, resulting in the formation of
functional peroxisomes (Knoops et al, 2014). Such PPVs were also recently identified in
S. cerevisiae pex3 cells (Wroblewska et al, 2017). Finally, work from Sugiura et al.
suggested that peroxisomes can derive from the mitochondria in mammalian cells
lacking Pex3p (Sugiura et al, 2017). Hence, the mechanisms of de novo peroxisome
formation are still under investigation.
Most observations on the de novo formation of peroxisomes are derived from cells
lacking Pex3p and to date, it has not been reported that Pex3p targets to the ER in wild
type (WT) cells. This has led to the suggestion that de novo formation of peroxisomes is
not the main mechanism by which new peroxisomes are made in WT cells and instead,
new peroxisomes derive from the growth and division model (Motley & Hettema, 2007).
In this model (Fig. 1), PMPs and MATs are synthesized in the cytosol and are
Introduction ONE
11
post-translationally targeted directly to pre-existing peroxisomes (for details on the
import processes, see the section Protein import into peroxisomes). At a certain point,
peroxisomes then divide in a process called fission (see below) to produce new
peroxisomes, that will subsequently import PMPs and MATs to become mature and fully
functional.
Fig 1. Schematic models of de novo peroxisome biogenesis in yeast.
(Upper) The left part represents ER-dependent peroxisome formation in cells lacking
Pex3p. In this model, PMPs first target to the ER and are subsequently sorted into two
heterotypic vesicles, the fusion of which in a Pex1p / Pex6p dependent manner generates
nascent peroxisomes. Through the import of MATs, nascent peroxisomes eventually grow
into mature ones. The right part represents an alternate model in which pre-peroxisomal
vesicles (PPVs) exist in cells lacking Pex3p. Upon reintroduction, Pex3p targets to PPVs
directly and facilitates the import of other PMPs in a Pex19p-dependent manner. When the
complete set of PMPs are present, the import of MATs allows the nascent peroxisome to
mature into a fully functional organelle.
(Lower) A schematic representation of the growth and division model in yeast. After
sufficient import of MATs has occurred, the mature peroxisome is ready to divide. To
initiate fission, an amphipathic α-helix of Pex11p inserts into the peroxisomal membrane
to elongate part of the membrane. High curvature membrane regions attract Fis1p, which
ONE Introduction
12
subsequently recruits Dynamin-related proteins (DRPs) like Dnm1 to the fission site. The
elongated region then undergoes constriction, though which factors are involved remains
unclear. At last, the DRPs finish the scission in a GTP-dependent manner. The daughter
peroxisome then grows in size by importing MATs and PMPs until stimulated to divide,
completing the cycle (see section on Peroxisome fission for more details on the process or
division).
Having said this, the PMP Pex16p appears to travel via the ER prior to targeting to
peroxisomes in WT mammalian cells (Kim et al, 2006), which would contradict the
hypothesis that the growth and division model is the main way in which new
peroxisomes are made in WT cells. In addition, studies in the parasite Trypanosoma
brucei proposed a model where extracellular glucose levels determined whether the
growth and division or the de novo mechanism facilitates glycosome biogenesis (Bauer
& Morris, 2017). Glycosomes (a type of peroxisome involved in glucose metabolism in
this organism) appear to favour the growth and division model in high extracellular
glucose concentrations whereas they favoured de novo biogenesis under low glucose
concentrations.
It seems therefore safe to assume that one model on the biogenesis of peroxisomes
does not fit all the observations and it is indeed highly likely that multiple pathways
exist to maintain the number of peroxisomes in the cell. Probably these mechanisms are
utilized depending upon circumstance and one may be preferred over the other under
certain conditions or in certain cell types.
3. Peroxisome fission
In the growth and division model, a mature and functional peroxisome can be
asymmetrically divided to form two peroxisomes in a process known as peroxisomal
division or fission. Fission can occur as response to external stimuli, such as is the case
when H. polymorpha yeast cells grown on glucose (a condition that does not require
peroxisome function) are shifted to methanol containing media. Because peroxisomes
are required to metabolise methanol, these cells rapidly increase the peroxisome
population, in order to deal with this challenge. Fission is also important to keep the
number of peroxisomes per cell steady, replacing old and worn out peroxisomes that are
degraded via pexophagy (see section Pexophagy).
Current models suggest that peroxisomal fission is a three-step process; peroxisome
remodelling/elongation, membrane constriction and scission. The first step is mediated
by the PMP Pex11p. Pex11p was the first factor identified that controls peroxisomal
Introduction ONE
13
fission. The deletion of PEX11 results in fewer and larger peroxisomes in cells while its
overexpression led to increased number of small peroxisomes (Erdmann & Blobel, 1995;
Marshall et al, 1995). S. cerevisiae contains a single copy of PEX11 (Erdmann & Blobel,
1995) while three PEX11 genes have been identified in mammalian cells (PEX11α, β,
and γ) (Schrader et al, 1998; Tanaka et al, 2003) and five PEX11 copies are present in
Arabidopsis thaliana (Orth et al, 2007). It is believed that these different versions of
Pex11p fulfil different roles in peroxisome fission or are required at different stages
(Huber et al, 2012). Recent work has shed light on the molecular function of Pex11p in
peroxisome fission, demonstrating that Pex11p initiates the membrane
remodelling/elongation step by inserting an amphipathic α-helix into the peroxisome
membrane, to initiate curvature (Koch et al, 2010; Opalinski et al, 2010). Furthermore,
many Pex11p proteins are known to form dimers or even higher order oligomeric
complexes and it is thought that these interactions are important in the elongation step
(Su et al, 2018). Several Pex11-like proteins have also been described, including Pex25p
in S. cerevisiae and H. polymorpha, Pex27p in S. cerevisiae and GIM5A and GIM5B in
trypanosomes (Williams & van der Klei, 2014). The role of these Pex11-like proteins in
peroxisomal fission remains largely unknown.
The second step in the fission process, the constriction step, is not well understood
and we know little about which proteins are involved and the mechanisms that govern
constriction. Some data may indicate that Pex11p may be involved in this step during
peroxisomal fission in mammalian cells (Schrader et al, 2016), but further work is
required before the first mechanistic insights become clear.
Scission, the final step in fission, requires dynamin-related proteins (DRPs). DRPs
are large GTPases that utilize GTP hydrolysis to severe the “daughter” peroxisome from
the “mother”. Drp1 in humans and Dnm1p in H. polymorpha are the DRPs required for
peroxisome fission in these organisms (Koch et al, 2003; Nagotu et al, 2008b). On the
other hand, two DRPs control fission in S. cerevisiae; Dnm1p (under peroxisome
inducing condition) and Vps1p (under peroxisome repressing condition) (Hoepfner et al,
2001; Koch et al, 2003; Kuravi et al, 2006). Interestingly, Pex11p also plays an
important role in the final step of the fission process, by activating the GTPase Dnm1p
(Williams et al, 2015), which demonstrates the interconnected nature of the fission
process and the players involved.
In addition to Pex11p and the DRPs, several other factors are involved in
peroxisomal fission, including Fis1p (Kobayashi et al, 2007; Motley et al, 2008), Mdv1
in yeast (Motley et al, 2008; Nagotu et al, 2008a) and MFF in humans (Itoyama et al,
2013; Koch & Brocard, 2012). The contribution these factors have to the peroxisomal
ONE Introduction
14
fission process are not well understood (Schrader et al, 2016; Schrader & Fahimi, 2008)
but they could be involved in recruiting DRPs to sites of membrane elongation or in
facilitating release of DRPs from the membrane after scission (Schrader et al, 2016;
Schrader & Fahimi, 2008). However, both Fis1p and MFF interact with Pex11p
(Itoyama et al, 2013; Koch & Brocard, 2012), which could suggest an earlier role in the
fission process.
4. Pexophagy – wholesale degradation of peroxisomes
New peroxisomes can be made either de novo or through peroxisomal fission.
Peroxisomal homeostasis however, is not only determined by the production of new
peroxisomes but also by the removal of older or damaged ones. Peroxisome removal
occurs via autophagy. Autophagy is an evolutionary conserved process that degrades
macro-molecules and organelles and is often initiated to recycle cellular components
that are not required or to remove damaged ones. The autophagic pathway that targets
peroxisomes for degradation is known as pexophagy (Eberhart & Kovacs, 2018).
There are two kinds of pexophagy: macro-pexophagy and micro-pexophagy (Farré
& Subramani, 2004; Tuttle & Dunn, 1995). During macro-pexophagy, a phagophore
assembly site (PAS) forms in the cell and from this PAS a double membrane originates
to engulf a cargo peroxisome into a double-membrane vesicle known as the
autophagosome. The autophagosome then fuses with the vacuole (or lysosome in
mammalian cells), to release the cargo into the vacuolar/lysosomal lumen, where the
peroxisomal membrane and proteins are degraded by the hydrolases that reside in the
vacuole/lysosome (Eberhart & Kovacs, 2018). Micro-pexophagy, on the other hand,
involves an invagination of the vacuole/lysosome membrane to engulf a group of
peroxisomes directly. Before complete engulfment of the peroxisomes occurs, the
micro-pexophagy-specific membrane apparatus (MIPA) forms, which
mediates fusion between the tips of the invaginating vacuole/lysosome
(Sakai et al, 2006). Once engulfed, peroxisomes are degraded in the vacuole/lysosome
in the same manner as in macro-autophagy. Both macro- and micro-autophagy are
orchestrated by autophagy-related (Atg) proteins.
In yeast, pexophagy can be triggered by a shift in nutrient conditions. When H.
polymorpha cells growing on methanol (peroxisome inducing) are treated with glucose
or ethanol (peroxisome repressing), the macro-pexophagy pathway degrades all but one
of the peroxisomes present in the cell (van Zutphen et al, 2008a). This is likely to occur
because peroxisomes are energetically expensive and are not required for growth on
glucose. Confusingly, the same happens in methanol-grown P. pastoris cells treated with
Introduction ONE
15
glucose yet pexophagy under these conditions in this organism occurs via the
micro-autophagy pathway (Farré & Subramani, 2004). Damaged H. polymorpha
peroxisomes are also subjected to degradation via macro-autophagy (Kiel et al, 2003). In
S. cerevisiae macro-pexophagy can be triggered when cells are subjected to nitrogen
starvation (Hutchins et al, 1999; Motley et al, 2012), causing cells to degrade
peroxisomes in order to obtain the nitrogen required to survive. In addition, in S.
cerevisiae the loss of the peroxisomal AAA-ATPase components Pex1p, Pex6p or the
PMP Pex15p leads to the accumulation of ubiquitinated Pex5p at the peroxisomal
membrane (see section Mechanism of peroxisomal matrix protein import) and
subsequently the macro-pexophagic degradation of peroxisomes (Nuttall et al, 2014).
Comparably, macro-pexophagy in mammals can also be triggered through loss of the
peroxisomal AAA-ATPase components or the accumulation of ubiquitinated Pex5p on
the peroxisomal membrane (Law, 2017) but also by several stress conditions including
hypoxic stress (insufficient oxygen availability), oxidative stress, serum/ amino acid
depletion and nutrient deprivation (Eberhart & Kovacs, 2018).
Of the two types of pexophagy, the better understood is macro-pexophagy. There
are four main steps in macro-pexophagy: the recognition of a peroxisome for
degradation, the formation of the PAS/autophagosome, fusion with the
vacuole/lysosome and the degradation of the peroxisome by vascular/lysosomal
hydrolases. In S. cerevisiae, the cytosolic C-terminal domain of Pex3p is first recognized
by the autophagy receptor Atg36p (Motley et al, 2012) (Fig. 2). The kinase Hrr25p then
phosphorylates Atg36p, which increases its interaction with Atg11p and Atg8p (Motley
et al, 2012). Atg11p is an essential protein in selective pexophagy in yeasts and serves as
a scaffold protein in the assembly of the PAS by binding to autophagy receptors, Atg17p
and Atg1p (Farré & Subramani, 2016). Atg17p in turn recruits other Atg proteins to the
PAS (Liu & Klionsky, 2016) while Atg1p is a Serine/ threonine protein kinase required
for the formation of the autophagosome (Stromhaug & Klionsky, 2001). The binding of
Atg36p to Atg8p is involved in autophagosome formation (Farré et al, 2013) and brings
the PAS to the peroxisomal membrane. Atg8p is an ubiquitin-like protein that is
conjugated to phosphatidylinositol lipids in the membrane of the phagophore (Klionsky
& Schulman, 2014; Noda & Inagaki, 2015). Recruitment of the
Atg8-phosphatidylinositol conjugate to the PAS requires Vps34p (Grunau et al, 2010).
Once fully assembled the phagophore then elongates, due to the action of the Atg8p
-Atg1p complex, to surround the peroxisome and forms the autophagosome. The fusion
of the autophagosome with the vacuole requires the action of several SNARE (Soluble
NSF Attachment Protein Receptor) proteins such as Sso1p/Sso2p and Sec9p (Nicholson
ONE Introduction
16
et al, 1998).
Fig. 2 Model of the formation of the phagophore in yeast.
(Left) In S. cerevisiae pexophagy, the Atg36p receptor first recognizes Pex3p. Next, the
kinase Hrr25p phosphorylates Atg36p, allowing it to recruit Atg8p and the scaffold protein
Atg11p. Atg11p further binds to the Atg17p scaffold complex and the Atg1p kinase
complex. (Right) To initiate pexophagy in H. polymorpha, Pex3p is ubiquitinated and
degraded via the UPS, which is likely to allow Pex14p to be recognized by an unidentified
autophagy receptor, to initiate pexophagy. Pdd1p is involved in the initial sequestration of
the peroxisome while Atg25p and Atg11p are required in the PAS. Atg1p and Atg8p are
further required to bring the phagophore closer to the peroxisome. Pdd2p is involved in the
later fusion with vacuole.
In H. polymorpha, glucose-induced macro-pexophagy is initiated by the
ubiquitination and degraded of Pex3p via the ubiquitin-proteasome system (UPS, see
section Ubiquitin-proteasome system) (Bellu et al, 2002; Williams & van der Klei,
2013a) (Fig. 2). Hazra et al. showed that Pex3p is involved in the association of
importomer complex (see section Mechanism of peroxisomal matrix protein import)
(Hazra et al, 2002). Hence, Pex3p removal is hypothesized to lead to the dissociation of
this complex (Leão & Kiel, 2003; Monastyrska & Klionsky, 2006) and the exposure of
the N-terminal region of the PMP Pex14p, a step that is required for pexophagy to
proceed (Bellu et al, 2001; van Zutphen et al, 2008b). Exposure of this region of Pex14p
recruits an as yet unknown autophagic receptor to the peroxisome. In addition, Pdd1p,
which is a homologue of S. cerevisiae Vps34p, is assumed to be involved in the initial
sequestration of peroxisome (Kiel et al, 1999). Similar to in S. cerevisiae, Atg11p acts as
scaffold protein while Atg1p and Atg8p are involved in the phagophore elongation step
Introduction ONE
17
(Monastyrska et al, 2005; Noda & Fujioka, 2015; Suzuki & Noda, 2018). In addition,
Atg25p is co-localized with Atg11p and it is likely involved in the formation of the
pre-autophagosomal structure.
In mammalian cells, macro-pexophagy can be initiated by the presence of
ubiquitinated proteins on the surface of the peroxisome (Law, 2017; Sargent et al, 2016).
Mammalian macro-pexophagy requires the ubiquitin-binding autophagy receptors
NBR1 and SQSTM1 (also termed p62) to connect the phagophore to the peroxisome
requiring degradation (Mancias & Kimmelman, 2016). Both these receptors contain an
LC3-interacting domain, allowing them to associate with the phagophore as well as
ubiquitin-association domains that bind to ubiquitinated proteins on the surface of the
peroxisome (Kirkin et al, 2009). LC3 is a family of Atg8p like proteins in mammalian
cells that, similar to Atg8p, are conjugated to phospholipids in the membrane of the
phagophore and are required for the formation of the autophagosome.
Defects that result in the accumulation of ubiquitinated Pex5p on the peroxisomal
membrane trigger NBR1-dependent macro-pexophagy (Deosaran et al, 2013; Subramani,
2015) (Fig. 3). However, starvation-induced macro-pexophagy can also be induced by
the presence of an ubiquitinated protein on the peroxisomal membrane. Recently,
Sargent et al. demonstrated that both Pex5p as well as the fatty acid transporter PMP70
(and possibly other PMPs) can be ubiquitinated by Pex2p in cells under amino acid
starvation conditions (Sargent et al, 2016). Amino acid starvation activates repressors of
tuberous sclerosis complex 1 (TSC1), TSC2 and Ras homolog enriched in brain (RHEB).
TSC1, TSC2 and RHEB are regulators of the mechanistic target of rapamycin complex 1
(mTORC1). The inhibition of mTORC1 results in an increased ubiquitination of Pex5p
and PMP70 by Pex2p, which is turn facilitates the recruitment of NBR1and the
formation of the phagophore.
ONE Introduction
18
Fig. 3 Model of the formation of the phagophore in mammalian cells.
(Left) Pexophagy caused by defects in the AAA-ATPases Pex1p/Pex6p: Ubiquitinated
Pex5p accumulates at the peroxisomal membrane and is recognized by the autophagy
receptor NBR1. NBR1 also interacts with LC3 proteins to connect the phagophore to the
peroxisome. (Right) Amino acid starvation inhibits mTORC1, which causes increased
ubiquitination of PMPs by Pex2p. The autophagic receptor NBR1 recognizes the
ubiquitinated PMPs and interacts with LC3 to form the PAS.
It is interesting to note that these recent reports on the role of ubiquitinated Pex5p
in pexophagy have shed new light on diseases resulting from deficiencies in Pex1p
(Nordgren et al, 2015). There is now strong evidence that patients with mutations in
PEX1 display symptoms because of an increase in macro-pexophagy caused by the
accumulation of ubiquitinated Pex5p on peroxisomes, rather than from a defect in the
import of matrix proteins into peroxisomes, as was previously thought.
5. Protein import into peroxisomes
Because peroxisomes lack DNA, they rely on several protein import pathways to obtain
the proteins required for function. Hence, peroxisomal protein import plays a crucial
role in determining peroxisome function.
5.1 Peroxisomal membrane protein (PMP) import into peroxisomes
There are two classes of sorting pathways for targeting PMPs to peroxisomes; Pex19p
dependent (known as Class-I) and Pex19p independent (known as Class-II). In Class-I
sorting, a PMP that is translated in the cytosol contains a membrane peroxisomal
targeting signal (mPTS). This mPTS is recognized by the cytosolic receptor protein
Pex19p (Jones et al, 2004) through the C-terminal region of Pex19p (Schueller et al,
2010). The Pex19p-PMP complex then targets to the peroxisomal membrane, where
Pex19p interacts with the PMP Pex3p via the N-terminal region in Pex19p (Sato et al,
2010; Schueller et al, 2010). Afterwards, the PMP is inserted into the membrane,
although the mechanism by which this occurs is still unclear (Hettema et al, 2014). A set
of PMPs were proposed to be sorted as Class-I PMPs, including the metabolite
transporters PMP22, PMP34, PMP70, the peroxisomal RING proteins, Pex11p and
Pex16p (Brosius et al, 2002; Jones et al, 2001; Jones et al, 2004; Sacksteder et al, 2000).
In the absence of Pex19p, many of the levels of these proteins are dramatically reduced
(Hettema et al, 2000), possibly because they are degraded if their targeting is inhibited.
In addition, Pex19p undergoes a post-translational modification called farnesylation at
Introduction ONE
19
its C-terminus, which induces a conformational change in Pex19p and facilitates the
recognition of conserved side chains in PMPs (Emmanouilidis et al, 2017). In S.
cerevisiae mutants blocking Pex19p farnesylation, levels of the RING proteins, Pex11p
and Pxa1p (a PMP involved in fatty acid transport) were dramatically reduced
(Rucktaschel et al, 2009), indicating that Pex19p farnesylation is important for Pex19p
function.
The Class-II PMPs are targeted to peroxisome via a different mechanism but
currently we know very little about this mechanism and also which PMPs can be
described at Class-II is unclear. Some reports have suggested that Class-II PMPs target
to peroxisomes via the ER and because under certain conditions Pex15p (Lam et al,
2010), Pex8p (van der Zand et al, 2010), Pex13p (van der Zand et al, 2010) and Pex3p
(Kim et al, 2006) in S. cerevisiae have been observed in the ER, these proteins were
classed as Class-II PMPs. However, many of these observations were based on work in
pex3 cells which were assumed to lack functional peroxisomes (Baerends et al, 1997).
The recent observation that H. polymorpha pex3 and pex19 cells as well as S. cerevisiae
pex3 cells contain PPVs (see section Peroxisome Biogenesis) that harbour a subset of
PMPs (including Pex8p, Pex13p, Pex14p, Pex15p, Pex17p, Pex25p and Pex22p
(Knoops et al, 2014; Otzen et al, 2004; Wroblewska et al, 2017)) indicates that it is not
clear whether these proteins target to peroxisomes via the ER or via a different
mechanism.
5.2 Mechanism of peroxisomal matrix protein (MAT) import
MATs are synthesized, folded and, when required, oligomerize in the cytosol prior to
being imported into peroxisomes. The import of MATs, similar to PMPs, relies on
peroxisomal targeting signals (PTSs). These signals are recognised by receptor proteins
in the cytosol and allow the proteins containing them to be targeted to peroxisomes.
Generally, most MATs possess a PTS type-1 (PTS1) while a small portion of MATs have
a PTS2 sequence. The original definition of the PTS1 sequence was a tri-peptide with
the consensus sequence S-A-C/ K-R-H/ I-L at the extreme C-terminus (Gould et al,
1987). However, later work demonstrated that up to the last 10 amino acids of the MAT
play an important role in recognition by the receptor protein (Otera et al, 1998). The
PTS1 is recognized by the receptor protein Pex5p (Gatto et al, 2003) (Fig. 4), although a
recent study demonstrated that Pex9p, a Pex5-like protein, is a novel peroxisomal import
receptor for certain PTS1 proteins in S. cerevisiae cells (Effelsberg et al, 2016). Pex5p
binds to the PTS1 sequence via its C-terminal Tetratricopeptide repeat (TPR) domain
(Gurvitz et al, 2001). The N-terminal region of Pex5p is involved in the docking and
ONE Introduction
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receptor recycling steps of import (see below).
The PTS2 sequence is an N-terminal signal with the consensus sequence
R-(L/V/I/Q)-X-X-(L/V/I/H)-(L/S/G/A)-X-(H/Q)-(L/A) (Kunze & Berger, 2015;
Lazarow, 2006; Petriv et al, 2004). PTS2-containing proteins are recognized by the
cytosolic receptor Pex7p. However, unlike Pex5p, which is able to facilitate the targeting
of PTS cargo proteins to peroxisomes independently, Pex7p requires an additional,
co-receptor protein (Fig. 5). This function is fulfilled by members of the Pex20p family
in yeasts (Schliebs & Kunau, 2006) whereas in mammalian cells, an isoform of Pex5p
(Pex5L) is required for Pex7p to target PTS2-containing proteins to peroxisomes
(Braverman et al, 1998; Matsumura et al, 2000). In PTS2 import, Pex7p is responsible
for binding to the cargo protein while the co-receptor is required for docking and (co-)
receptor recycling (see below).
Apart from canonical PTS1 and PTS2 proteins, proteins without a typical PTS
signal can also be imported into peroxisomes. Such proteins may bind to another one
containing a typical PTS, which is recognized by the corresponding receptor protein and
imported. S. cerevisiae Pnc1p, which lacks a PTS, is imported into peroxisomes through
its interaction with the PTS2 protein Gpd1p via such a “piggy-backing” mechanism
(Kumar et al, 2016). However, piggy-backing cannot explain the import of certain
non-PTS1/2 containing proteins into peroxisomes. Peroxisomal
hydratase-dehydrogenase-epimerase (Fox2p) and catalase A (Cta1p) in S. cerevisiae
both contain a PTS1 sequence yet they can be imported into peroxisomes by Pex5p
independently of this signal (Rymer et al, 2018). Furthermore, acyl-CoA oxidase (Pox1p)
in S. cerevisiae lacks a PTS1 but it is imported into peroxisomes in a Pex5p-dependent
manner (Klein et al, 2002). The targeting of non-PTS1 proteins to peroxisomes via
Pex5p has led to the suggestion that a PTS3 pathway exists although a PTS3 consensus
sequence has not been identified yet. Finally, Aat2p in the yeast H. polymorpha lacks a
recognizable PTS sequence but it can target to peroxisomes in a Pex5p and Pex7p
independent manner (Thomas et al, 2018). The targeting of Aat2p instead requires the
PTS2 co-receptor Pex20p. Based on these observations, it seems very likely that there
are as yet uncharacterized PTS signals.
After the recognition of MATs in the cytosol, the cargo-receptor complex then
targets to the peroxisomal membrane where it docks. The peroxisomal docking complex
consists of the PMPs Pex13p and Pex14p. Another PMP, Pex17p, is also part of the
docking complex in yeast and a recent study showed that Pex17p is required for the
assembly of high molecular weight complexes between Pex14p and the Dynein light
chain protein Dyn2p, which are important for MATs import (Chan et al, 2016) although
Introduction ONE
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the role of Pex17p in MAT import is still rather enigmatic.
Pex5p interacts directly with both Pex14p and Pex13p (Urquhart et al, 2000) while
Pex13p and Pex14p also interact directly with each other at multiple points (Williams &
Distel, 2006). The Pex5p-Pex14p interaction is facilitated by WxxxF/Y motifs present in
the N-terminal region of Pex5p (Otera et al, 2002). Such motifs can be found in all Pex5
proteins to date, and are also present in Pex20p family members, indicating that
common mechanisms govern the import of both PTS1 and PTS2 proteins. Pex14p
interacts with Pex5p through two different regions; its N-terminal domain as well as the
C-terminal region and both are required for PTS1 protein import (Williams et al, 2005).
Pex7p, the PTS2 receptor protein also binds to the C-terminal region of Pex14p
(Niederhoff et al, 2005), again indicating the conservation between the mechanisms of
PTS1 and PTS2 protein import.
The Pex5p-Pex14p interaction is enhanced in the presence of a PTS1 cargo protein
while the Pex5p-Pex13p interaction is stronger in the absence of a cargo protein
(Urquhart et al, 2000). This has led to a model where Pex14p acts as the first point of
contact for the Pex5p-Cargo complex and that Pex13p is actually involved in a
post-docking function (Bottger et al, 2000). However, Pex5p and Pex14p can bind to the
SRC Homology 3 (SH3) domain of Pex13p simultaneously (Pires et al, 2003),
indicating that the individual roles played by Pex13p, Pex14p and Pex5p in the import
process are very strongly interconnected.
Fig 4. Model depicting the steps of PTS1 protein import into peroxisomes.
(1) MATs harbouring a PTS1 signal at the C-terminus are synthesized in the cytosol and
recognized by the cytosolic receptor Pex5p. (2) The receptor-cargo complex targets to the
docking complex composed of Pex13p and Pex14p (with its co-partner Pex17p in yeast) at
the peroxisomal membrane. (3) A transient import pore is formed consisting of the Pex5p
receptor and the docking proteins. (4) After the cargo translocation and cargo release, the
ONE Introduction
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receptor is ubiquitinated and (5) either recycled by the AAA-ATPase complex back to the
cytosol for next round of import or degraded by the proteasome.
In order to translocate a cargo protein across the peroxisomal membrane and into
the matrix, a pore is needed (Fig. 5). Such a pore needs to be large enough to
accommodate folded and even oligomeric proteins but at the same time the pore cannot
allow small molecules and proteins to escape out of the peroxisome. To date no
peroxisomal pore has been observed using techniques such as electron microscopy
(Meinecke et al, 2016), which has led to the hypothesis of a transient import pore that
forms when required and then dissociates after cargo protein import. Evidence to
support this hypothesis comes from elegant studies using electrophysiological
approaches (Montilla-Martinez et al, 2015). In these reports, the authors utilized purified
components to reconstitute the import pore or “importomer”, demonstrating that a
complex of Pex5p, cargo and Pex14p was sufficient to form a pore in a membrane
capable of opening and closing (Montilla-Martinez et al, 2015). The size of the pore that
formed was largely determined by cargo protein size, indicating that the importomer is
dynamic in nature and can adapt according to the type of cargo being translocated. In
follow on studies, the same authors identified a distinct PTS2 specific pore that
contained the PTS2 co-receptor Pex18p as well as Pex14p and Pex17p
(Montilla-Martinez et al, 2015), which led to the hypothesis that the import of PTS1 and
PTS2 proteins does in fact not converge at the peroxisomal membrane, as was
previously thought (Hettema et al, 1999). Together, these data indicate that complexes of
the receptor, cargo and Pex14p (with Pex17p for the PTS2 pore) were sufficient for pore
forming activity in vitro. However, where Pex13p and, to a certain extent Pex17p, fit
into the model describing receptor docking and translocation still remains to be
determined.
One aspect of the MAT import process that we know very little about is that of
cargo release into the peroxisomal matrix. In yeast, a role in cargo release has been
attributed to the protein Pex8p, for two reasons; Pex8p is able to bind to Pex5p-cargo
complexes in vitro and facilitate release of the cargo protein from the complex (Rehling
et al, 2000b) and Pex8p is present on the inside of the peroxisomal membrane (Deckers
et al, 2010). Pex8p also binds to the docking factor Pex13p as well as to PMPs involved
in receptor recycling (see below), which brings both the docking and receptor recycling
steps in the import process together (Agne et al, 2003). However, Pex8p had to date not
been identified in mammals (Smith & Aitchison, 2013a), which has led some to question
this potential role in cargo release. It is possible that Pex14p plays a role (either together
Introduction ONE
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with Pex8p or alone) in the cargo dissociation process (Lanyon-Hogg et al, 2014) while
the fact that Pex13p binds more tightly to Pex5p without cargo may also suggest a role
for Pex13p in cargo release. Furthermore, recent reports suggest that the interaction
between Pex5p and cargo may be redox-regulated (Ma et al, 2013), leading to the
hypothesis that cargo release could be facilitated by the reducing environment of the
peroxisomal lumen (Ma et al, 2013), although a later study reported that redox
conditions did not impact on Pex5p-cargo interactions in their experimental setup
(Walton et al, 2017).
Fig 5. Distinct pores for peroxisomal import of PTS1 and PTS2 proteins
(Montilla-Martinez et al, 2015).
The figure shows two kinds of PTS-specific pores at the peroxisomal membrane for MATs
import. (left) A PTS1 import pore contains Pex5p and Pex14p as major components. (right)
A PTS2 import pore contains PTS2 co-receptor Pex18p, Pex14p and Pex17p as major
components.
After cargo translocation across the peroxisomal membrane and cargo release, the
receptor protein (or receptor/co-receptor complex) is recycled to the cytosol, to take part
in another round of import. Recycling of the (co-) receptor requires the receptor to
undergo a post translational modification called mono-ubiquitination. Ubiquitination
involves the attachment of the 8kDa protein ubiquitin to a substrate and the attachment
of a single ubiquitin molecule to the substrate is known as mono-ubiquitination whereas
attachment of a chain of ubiquitin molecules is referred to as poly-ubiquitination (see
section The ubiquitination cascade). Mono-ubiquitination occurs on a well conserved
cysteine residue very close to the N-terminus of Pex5p/Pex20p family members (Leon
& Subramani, 2007; Williams et al, 2007). In yeast it depends on the action of Pex4p
(together with its membrane anchor Pex22p) (Koller et al, 1999; Van der Klei et al,
ONE Introduction
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1998), a peroxisome-associated ubiquitin conjugating enzyme (E2), and a complex of
Pex2p, Pex10p and Pex12p (El Magraoui et al, 2012), three PMPs that all contain a
really interesting new gene (RING) domain (Borden & Freemont, 1996) and function as
ubiquitin ligases (E3s). The RING proteins are also involved in Pex5p
mono-ubiquitination in mammals but a different E2 (members of the Ube2D family) is
required (Grou et al, 2008). The actual recycling step, the removal of the receptor out of
the membrane, requires the action of Pex1p and Pex6p, two AAA-ATPases that form a
hetero-hexameric complex, and the PMP Pex15p (Pex26p in mammals), which is
required to bring the mostly cytosolic Pex1p/Pex6p complex to the peroxisomal
membrane (Fujiki et al, 2008). The Pex1p/Pex6p complex recognises the
mono-ubiquitinated (co-) receptor protein and uses ATP hydrolysis to extract it from the
peroxisomal membrane (Platta et al, 2008). During the membrane extraction process, the
ubiquitin is removed from mono-ubiquitinated Pex5p (and likely Pex20p family
members) by Ubp15p in yeast (Debelyy et al, 2011) and USP9X in mammals (Grou et al,
2012), which allows the protein to take part in another round of import.
In certain cases, the (co-) receptor proteins can undergo poly-ubiquitination. This is
mostly seen in mutants lacking PEX4 or PEX1/PEX6 or when the conserved cysteine
residue in the (co-) receptor is mutated (Léon & Subramani, 2007; Williams et al, 2007).
(Co-) receptor poly-ubiquitination often leads to degradation of the (co-) receptor via the
proteasome (see section The proteasome), likely to stop the accumulation of proteins
on the peroxisomal membrane that are unable to recycle. Poly-ubiquitination of the (co-)
receptors, which occurs on conserved lysine residues in the N-terminal region (Liu &
Subramani, 2013), also requires the RING protein complex (Platta et al, 2009; Williams
et al, 2008) but some substrate specificity is observed when it comes to the E2 involved.
Pex5p and Pex18p poly-ubiquitination in S. cerevisiae require Ubc4p yet Pex20p
poly-ubiquitination in P. pastoris requires Pex4p (Liu & Subramani, 2013; Williams et
al, 2008). The E2 responsible for Pex5p poly-ubiquitination is currently unknown but it
remains feasible that members of the Ube2D family of E2 are involved in both the
mono- and poly-ubiquitination of Pex5p (Stewart et al, 2016).
Removal of the poly-ubiquitinated (co-) receptors out of the peroxisomal
membrane is required for them to be degraded via the proteasome. In S. cerevisiae it is
believed that this is facilitated by the Pex1p/Pex6p complex (Platta et al, 2008) yet the
observation that Pex5p is almost undetectable in P. pastoris cells lacking Pex1p or
Pex6p (Collins et al, 2000) would suggest that alternative mechanisms exist to remove
poly-ubiquitinated proteins from the peroxisomal membrane and target them for
degradation via the proteasome.
Introduction ONE
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Finally, a recent report demonstrated that an alternative form of Pex5p
mono-ubiquitination in mammals protects Pex5p from degradation via the proteasome
(Wang et al, 2017). This modification required the E3 ligase TRIM37 and members of
the Ube2D family of E2s and occurs in the C-terminal region of Pex5p. The mechanism
underlying how this form of mono-ubiquitination protects Pex5p from proteasomal
degradation remains to be determined but together with the reports mentioned above, it
clearly demonstrates the important role ubiquitin and ubiquitination plays in peroxisome
biology.
6. Protein degradation – the Ubiquitin-proteasome system
The ubiquitin proteasome system (UPS) is the major protein degradation pathway in
eukaryotic cells (Bett, 2016). The UPS pathway consists of the ubiquitination cascade
and the proteasome.
6.1 The ubiquitination cascade
In the ubiquitination process, a ubiquitin molecule, a 76-amino acid globular protein, is
attached to a substrate protein, usually on a lysine residue in the substrate (Swatek &
Komander, 2016). Attachment of a single ubiquitin to a substrate is referred to as
mono-ubiquitination and mono-ubiquitination has been linked to several cellular
processes, such as regulating the substrates interactions with other proteins or in its
localisation (Pickart, 2001). However lysine residues in the ubiquitin molecule itself can
also be the target of ubiquitin attachment, resulting in the formation of ubiquitin chains,
which is referred to as poly-ubiquitination. Seven different types of ubiquitin chain can
be formed, based on seven internal lysine residues in ubiquitin (Table 1). Furthermore,
the C-terminus of one ubiquitin molecule can be attached to the N-terminal methionine
of another ubiquitin molecule, forming a linear poly-ubiquitination chain (Table 1).
Probably the most common form of poly-ubiquitin chain in the cell is linked via lysine
48 (K48) on ubiquitin. K48-linked poly-ubiquitinated substrates undergo proteasomal
degradation. The ubiquitin chain acts as a tag that allows the substrate to be transported
to the proteasome, for degradation. However, not all ubiquitination events are for
degradation and several non-proteolytic functions are regulated by the attachment of
different types of poly-ubiquitin chains. For example, K6-linked chains are involved in
DNA damage repair while K11-linked chains play a role in cell cycle regulation and
K27-linked chains are involved in T-cell development (Ikeda et al, 2010; McDowell &
Philpott, 2013).
ONE Introduction
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Linkage type Function/ Processes involved in
Linear Signal transduction
K6 DNA damage
K11 Cell cycle regulation,
membrane trafficking,
TNF signaling
K27 Mitophagy,
T-cell development,
signal transduction
K29 AMPK regulation
K33 AMPK regulation
TCR signaling
K48 Proteasomal degradation
K63 Signal transduction
Table 1. Functional roles of the different linkage types of polyubiquitination.
The ubiquitination cascade (Fig. 6), which facilitates the ligation of ubiquitin to a
substrate protein requires the sequential action of three enzymes (Hershko &
Ciechanover, 1998). It begins with a ubiquitin activating enzyme (E1, step-1), which
activates a ubiquitin molecule by conjugating the C-terminal Gly residue of ubiquitin
onto an active site cysteine in an ATP-dependent manner. The activated ubiquitin will
then be transferred to an active Cys residue of a ubiquitin-conjugating enzyme (E2,
step-2). Catalysed by a ubiquitin-protein ligase (E3, Step-3), ubiquitin is linked to the
ε-amino group of a lysine residue in the substrate protein. In the case that the substrate is
poly-ubiquitinated, this process is repeated, using a lysine residue in ubiquitin. The
ubiquitin cascade is pyramidal in organisation (Hochstrasser, 1996). Cells contain a
single E1, several E2s (~11 in yeast but around 35 in humans) and a larger number of
E3s. E3s provide much of the selectivity of ubiquitin-protein ligation and therefore
protein degradation (Hershko & Ciechanover, 1998) and many target specific substrates
or groups of substrates. It is estimated that yeast contains around 50 E3s while humans
are thought to possess maybe up to 1000 different E3s (Zheng & Shabek, 2017).
Introduction ONE
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Fig 6. Schematic overview over the enzymatic cascade catalyzing ubiquitination.
Ubiquitin is first activated by a ubiquitin-activating enzyme (E1) with ATP hydrolysis.
Next, the E1 transfers the ubiquitin to a ubiquitin-conjugating enzyme (E2), then with the
aid of a ubiquitin ligase (E3) which plays an important role in specifying the substrate,
ubiquitin is eventually transferred to a substrate. HECT-E3s conjugate the ubiquitin onto
an active site before attaching it to a substrate while RING-E3 serves as a bridge to
enable ubiquitin to be passed directly from the E2 to the substrate. Substrate proteins can
be either mono- or poly-ubiquitinated.
Two different types of E3 ligase are known, those of the RING family and those of
the HECT family. These different types of E3s utilize different mechanisms to transfer
ubiquitin to the substrate. A RING (Really Interesting New Gene) E3 contains a RING
finger domain, consisting of a C3HC4 amino acid motif (seven cysteines and one
histidine arranged non-consecutively) which binds to two zinc cations (Borden &
Freemont, 1996; Freemont et al, 1991). There are around 600 E3 enzyme from the
RING type in the human genome (Vittal et al, 2015). RING E3 ligases bind
simultaneously to an E2 with ubiquitin on its active site and an appropriate substrate,
which allows the ubiquitin to be transferred to the protein substrate (Hershko &
Ciechanover, 1998). HECT E3s, on the other hand possess a HECT (Homologous to the
E6-AP Carboxyl Terminus) domain, conjugate ubiquitin onto an active site in the HECT
domain and then transfer this ubiquitin to the protein substrate (Hershko & Ciechanover,
1998).
While many ubiquitination events require only an E3, certain substrates need an
adaptor protein, to allow efficient transfer of ubiquitin from the E3. One such family is
the Cullins, which are scaffold proteins that provide support for E3 ligases (Petroski &
Deshaies, 2004; Petroski & Deshaies, 2005). Furthermore, some of these adaptor
proteins have been assigned the name E4 and they work in association with E1, E2 and
E3 enzymes by catalysing the extension of ubiquitin chains (Hoppe, 2005). It is still
ONE Introduction
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under discussion whether it is a new class of enzymes, or a subclass of E3. The ubiquitin
fusion enzyme Ufd2 is one of the few identified E4s so far (Koegl et al, 1999) and
belongs to a family of proteins in eukaryotes that contain a conserved U-box at their
C-terminus, which is generally considered essential for E4 function (Hatakeyama &
Kei-ichi, 2003). A U-box is structurally related to the RING finger domain (Aravind &
Koonin, 2000; Tu et al, 2007).
Substrate ubiquitination is not a one way process and the removal of ubiquitin from
substrates (deubiquitination) can be as important as the ubiquitination process itself. The
deubiquitination of substrates is mediated by a deubiquitinase (DUB). DUBs are
enzymes that hydrolyze the isopeptide or peptide bond between the ubiquitin C-terminus
and the substrate (Mevissen & Komander, 2017). The DUBs can be categorized into two
families, a group of small proteins of ~30kD mainly for the removal of ubiquitin from
peptides and small adducts, like Yuh1 in yeast, and a group of larger proteins to cleave
ubiquitin off protein substrates (reviewed in (Hochstrasser, 1996)). The latter family of
DUBs are also termed as Ubps, including various large proteins of ~100kD which have
conserved Cys and His boxes (Wilkinson et al, 1995). Interestingly DUBs outnumber
E2s in the cell (e.g. 16 Ubps in S. cerevisiae compared to 11 E2 enzymes (Hochstrasser,
1996; Ye & Rape, 2009)), indicating their importance in the cell. Indeed, mutations in
the DUB Faf, the gene of which is required for eye development in Drosophila, leads to
null phenotypes in transgenic flies, demonstrating the importance of DUBs in biological
function (Huang et al, 1995). However, several yeast ubp mutants do not display a clear
phenotype, possibly because either these Ubps function under specific conditions or they
are redundant (Baker et al, 1992).
Furthermore, DUBs are not simply there for the negative regulation of
ubiquitination. DUBs help to generate ubiquitin monomers, required to keep the
intracellular pool of free ubiquitin sufficiently high to allow substrate ubiquitin to
proceed efficiently (Pickart & Rose, 1985). DUBs disassemble the ubiquitin chains from
E3 to prevent excessive binding and accumulation of inhibitory ubiquitin oligomers
(Hershko & Ciechanover, 1992). Furthermore, ubiquitinated substrates destined for
proteasomal degradation are deubiquitinated prior to degradation (Hu et al, 2005; Verma
et al, 2002), likely to stop the ubiquitin conjugate from blocking the proteasome during
the degradation process and also to allow the ubiquitin molecule to be recycled.
As can be seen, the ubiquitination cascade is a highly complex system that contains
many points at which substrate ubiquitination can be regulated and controlled
6.2 The proteasome – the protein waste disposal system in the cell
Introduction ONE
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The 20S proteasome is a huge, multi-subunit protease found in many organisms ranging
from the oldest bacteria (archaea), to modern plants and animals. The whole eukaryotic
20S proteasome is about 16 nm in height and has a diameter of about 10 nm (Tomisugi
et al, 2000). The structure of the 20S proteasome consists of four rings containing seven
subunits in each ring. The rings are arranged in the order of α-β-β-α (Fig. 7). In archaea,
there is only one type of α-subunit and one type of β-subunit and each β-subunit displays
comparable proteolytic activity while in eukaryotic cells, there are seven different types
of subunits found in the α-rings and β-rings (Fig. 7A-B) and only three β-subunits (β1,
β2 and β5) have proteolytic activity (Fig. 7C). Subunit β1 cleaves after acidic amino
acids, β2 after basic amino acids and β5 after neutral amino acids. The proteolytic
activity of β5 is considerably higher than that of β2 and β1. The inside of the 20S
proteasome is subdivided into three chambers (Fig. 7D), two antechambers form
between an α and a β ring, and one main proteolytic chamber formed between two β
rings. The gate through which substrates enter into the chambers is comprised of the last
ten amino acids of the N-terminus of subunits α2, α3 and α4. Structures of the 20S
proteasome have demonstrated that the N-terminus of subunit α3 blocks the gate and
currently it is not well understood how substrates pass through the gate of the 20S
proteasome (Jung & Grune, 2008).
Fig 7. The structure of proteasome.
(A) the ball model of Archaea proteasome. (B) the ball model of 20S part of proteasome in
eukaryotic cells, take yeast S. cerevisiae as example. (C) the view of a single β-ring of (B).
(D) the structure of eukaryotic proteasome, showing the 20S part.
By binding with different (often inducible) subunits or regulatory proteins, the 20S
proteasome upgrades itself and gains new functions or to change its substrate specificity
and activity (Jung & Grune, 2013). For example, the immunoproteasome (consisting of
two 11S and one 20S components and termed i20S) is fast acting and is involved in the
ONE Introduction
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immune response to pathogens or inflammatory processes (Piccinini et al, 2003;
Stratford et al, 2006) while the hybrid-proteasome (19S-20S-11S components) is
possibly involved in the production of oligo-peptides for MHC-I presentation in immune
response.
The major form of the proteasome in eukaryotes is the 26S proteasome (two 19S
and one 20S components) and it is this form that facilitates the degradation of most
substrates of the UPS. The 26S proteasome can degrade natively folded proteins
whereas the 20S proteasome is only able to recognize and degrade proteins that are
already unfolded (DeMartino et al, 1994; Liu et al, 2002). This ability comes from the
19S component, a 700 kD protein complex consisting of six Rpt subunits (Rpt1-6) that
display ATPase activity and 13 non ATPase Rpn subunits (Rpn1-3, 5-13 and 15) that
captures ubiquitinated substrates, unfolds them and then feeds to the 20S proteolytic
core (Thrower et al, 2000). The poly-ubiquitin chain is removed by the action of a DUB
associated with the 19S component (Kim et al, 2018).
Unlike with the 20S proteasome, the mechanism by which substrates gain access to
the inner chamber of the 26S proteasome has been elucidated. The C-terminus region of
the 19S ATPases, which contain a specific HbYX (hydrophobic residue, tyrosine, X)
motif, inserts into the pockets between neighbouring alpha subunits. This interaction
induces a rotation in the alpha subunits and displacement of a reverse-turn loop that
stabilizes the open-gate conformation (Rabl et al, 2008). This binding stimulates the
opening of the gate of the 20S upon ATP binding to the ATPase subunits, similar to the
way in which a key in a lock opens a door (Smith et al, 2007).
6.3 The UPS-dependent degradation of organellar membrane proteins
The correct folding, location and amount of any protein is fundamentally important for
its function in the cell. This means that proteins that become misfolded or damaged,
mislocalized or are present in too high amounts may cause problems in the cell and it is
for this reason that pathways such as the UPS facilitate the degradation of unwanted
proteins. This also extends to the degradation of membrane proteins present on
organelles.
One of the most well studied pathways that targets organelle membrane proteins for
degradation is that of ER-Associated Degradation (ERAD), which targets ER membrane
proteins for ubiquitination and degradation by the proteasome. About one-fourth of
eukaryotic genomes encode for integral membrane proteins and the ER is the site of
initial assembly for a large number of them (Shao & Hegde, 2011). Because the folding
and correct assembly of membrane proteins is a challenge, the ERAD pathway ensures
Introduction ONE
31
that membrane proteins that become terminally unfolded do not accumulate in the ER
but are instead degraded. Likewise, ERAD also targets proteins that are incorrectly
glycosylated or damaged as well as a number of redundant ER membrane proteins.
Substrates of the ERAD pathway are first recognized as unwanted and
ubiquitinated by E2s and E3s. This is a part of the ERAD pathway that is still not well
understood. In certain cases substrate recognition occurs through the action of chaperone
proteins such as OS-9, XTP3-B and SEL1L (reviewed in (Hebert & Molinari, 2012)
while the E3s themselves also possess the capability to recognize substrates (Stein et al,
2014). In the case where redundant proteins are targeted for degradation, a “degron”
sequence in the substrate often allows the protein to be recognised and degraded (Ravid
et al, 2006; Smith et al, 2016). Such sequences often lack structure and it is thought that
they mimic unfolded domains and are recognised as misfolded proteins and
subsequently degraded (Ravid & Hochstrasser, 2008).
Two well conserved RING E3s in S. cerevisiae, Hrd1p and Doa10p, are involved in
the degradation of most yeast ERAD substrates (Bays et al, 2001; Swanson et al, 2001),
working with the E2s Ubc6p and Ubc7p (Bazirgan & Hampton, 2008) to ubiquitinate
substrates. After ubiquitination, the substrate membrane protein is extracted from the ER
membrane in an ATP-dependent retro-translocation process and delivered to the
proteasome, which is usually present in the cytosol, for degradation (Christianson & Ye,
2014; Erzberger & Berger, 2006; Sauer & Baker, 2011). In humans, at least four E3
ligases are involved in the ERAD pathway, including CHIP, RMA1, gp78 and HRD1
(similar to yeast Hrd1p) (Kawaguchi & Ng, 2007), working together with four E2s
(UBE2G1, -G2, -J1 and- J2) to promote substrate ubiquitination and degradation (Ye &
Rape, 2009).
Retro-translocation relies on the ATPase Cdc48p (p97 in mammalian cells), which
utilizes ATP hydrolysis to wrench the substrate membrane protein out of its favoured
environment, the ER membrane. Cdc48p also binds to a number of additional factors,
such as Npl4p and Ufd1p and it is thought that these are adaptor proteins that help in
substrate recognition (Meyer et al, 2000). In an interesting variation to the role of
Cdc48p in the retro-translocation step of ERAD, a recent report on the
ERAD-dependent degradation of the cadmium sensing protein Pca1p (Smith et al, 2016)
demonstrated that Cdc48 played a role in recruiting the 26S proteasome to the ER
membrane, to facilitate the degradation of Pca1. The authors suggested that such
mechanisms may enhance the efficiency by which Pca1 degradation proceeds while also
negating the requirement to protect the hydrophobic regions of Pca1 from the cytosol
while being transported to the proteasome. In addition, similar observations were
ONE Introduction
32
reported for a subset of additional ER membrane proteins and it will be interesting to
investigate further whether this is a general or specific mechanism for the degradation of
membrane proteins.
The ERAD pathway is only one of a number of pathways that target membrane
proteins for UPS-mediated degradation. Indeed, several years ago, Heo et al identified a
pathway that facilitates the degradation of membrane proteins on mitochondria exposed
to stress (Heo & Rutter, 2011). This pathway, which they termed Mitochondrial
Associated Degradation (MAD), also requires the ATPase Cdc48p as well as Vms1p, an
evolutionary conserved cytosolic protein that recruits Cdc48p to the mitochondria under
stress conditions, to facilitate degradation. Since this time, several reports have
identified additional substrates of the MAD pathway as well as MAD specific factors
required for the turnover of mitochondrial membrane proteins (Wu et al, 2016).
Likewise, membrane proteins present on chloroplasts can also be targeted for
degradation. In a recent paper, Ling et al. demonstrated that the chloroplast
membrane-bound RING E3 ligase SP1 was involved in the selective UPS-mediated
degradation of members of the Translocon at the Outer envelope of Chloroplasts (TOC)
complexes, which facilitate protein import into chloroplasts (Ling & Jarvis, 2015).
Degradation of these TOC components allows chloroplasts to reorganize their import
machinery, to regulate the import of proteins into chloroplasts.
In conclusion, the degradation of unwanted organellar membrane proteins is crucial
for organelle function but many questions still remain concerning how for example
substrates of these pathways are recognized and how the removal of the hydrophobic
regions of a membrane proteins is facilitated without generating disturbances to the
membrane itself.
6.4. Degradation of peroxisomal proteins
The wealth of information on the degradation of organellar membrane proteins from for
example the ER is in sharp contrast to what is known on the degradation of peroxisomal
membrane proteins (PMPs). To date, there are only two PMPs that are known to be
targeted for USP-mediated degradation: Pex3p in the yeast H. polymorpha (Williams &
van der Klei, 2013a) and Pex13p in plants (Pan et al, 2016). Methanol-grown H.
polymorpha cells exposed to glucose degrade all but one of their peroxisomes via
pexophagy (see above) and initiation of pexophagy requires that the PMP Pex3p is
ubiquitinated and degraded in a process involving the peroxisomal E3 ligase complex
and the UPS (Bellu et al, 2002; Williams & van der Klei, 2013a). In the case of plant
Pex13p, the RING E3 ligase SP1 was reported to localise not only to the chloroplast but
Introduction ONE
33
also the peroxisomal membrane and to facilitate UPS-mediated Pex13p degradation
(Pan et al, 2016), although the localisation of SP1 is still under discussion (Ling et al,
2017; Pan & Hu, 2018). While not confirmed, several reports in the literature suggest
that additional PMPs are targeted for degradation via the UPS. For example, levels of
the peroxisome inheritance factors Inp1p and Inp2p are regulated in a cell-cycle
dependent manner (Fagarasanu et al, 2006; Kumar et al, 2017). Furthermore,
ubiquitinated peptides of Pex14p have been found in S. cerevisiae (Mayor et al, 2007;
Seyfried et al, 2008; Tagwerker et al, 2006) and human cells (Kim et al, 2011),
suggesting that this PMP too undergoes UPS-mediated degradation. Clearly PMP
degradation pathways also exist but this field is still in its infancy.
However, it has been known for some time that the UPS plays a role in peroxisome
biology, through the degradation of poly-ubiquitinated Pex5p/Pex18p/Pex20p (see
above). In all cases the peroxisomal ubiquitination machinery was required, although the
mechanisms were varied. In addition, it was recently reported that the PTS2 co-receptor
Pex7p also undergoes UPS-mediated degradation in the yeast P. pastoris (Hagstrom et al,
2014) and in humans (Miyauchi-Nanri et al, 2014). The peroxisomal ubiquitination
machinery seemed not to be required for Pex7p degradation in either organism whereas
the cytosolic E3 ligase complex CRL4A (Cullin4A-RING Ub E3 ligase) was required
for Pex7p ubiquitination/degradation in humans. In both cases, the authors reported that
non-functional Pex7p was targeted for degradation, defining these degradation events as
quality control related.
Another example of quality control at the peroxisomal membrane concerns the
AAA-ATPase Msp1p. This membrane anchored protein targets to both peroxisomes and
mitochondria and seems to play a role in removing incorrectly targeted tail anchored
membrane proteins for degradation (Chen, 2014; Okreglak, 2014; Weir et al, 2017;
Wohlever et al, 2017). Currently it is not known whether Msp1p also targets other
classes of membrane proteins nor whether the UPS is involved in these degradation
events.
While it is clear that the peroxisomal ubiquitination machinery can target certain
peroxisomal proteins for UPS-mediated degradation, the role of Msp1p and CRL4A in
the degradation of peroxisomal proteins indicates that pathways targeting peroxisomal
proteins are integral into general cellular degradation systems and are not stand alone
pathways exclusively targeting peroxisomal proteins.
7. Peroxisomal proteomics
Cells adapt the protein content of peroxisomes depending on their metabolic
ONE Introduction
34
requirements because the proteins that are present in a particular peroxisome determine
its function, whether they are the enzymes of the different metabolic pathways housed
inside peroxisomes or the PMPs involved in the import of proteins or small molecules
(Hazra et al, 2002; Van den Bosch et al, 1992). Hence, obtaining information on which
proteins are present in peroxisomes at a given time or under a given condition provides
an invaluable insight into the role of peroxisomes in cell biology. Indeed, many
peroxisome functions have been determined using microscopy and/or biochemical
methods. However, in recent years the use of mass spectrometry (MS) to study
peroxisomal proteomics has led to the identification of many new peroxisomal proteins
and hence new peroxisome functions (Schäfer et al, 2001; Yi et al, 2002). This has
resulted in a better understanding of how peroxisomes are integrated into the metabolic
and regulatory networks in cells. New MS-based proteomics approaches are being
developed all the time, that allow for better sensitivity and the reduction of false
positives and it is fair to say that through the use of such techniques, new insights into
peroxisomal function are undoubtedly on the horizon.
8. Perspectives
While our understanding of the processes that regulate peroxisome functions has
increased dramatically over the last 10 years, there are still many things about these
processes that we do not understand. For example, do the growth and division and de
novo pathways work simultaneously in wild type cells and if so, how are they regulated
and coordinated under various conditions? In addition, how the targeting of peroxisomal
membrane proteins (PMPs) to peroxisomes is achieved is still poorly understood.
Finally several studies have indicated a role for the endomembrane system in
peroxisome biogenesis and PMP import while others refute this, demonstrating that we
as yet do not understand enough about these processes to derive one all-inclusive model
that describes all the available data.
Peroxisomal matrix proteins (MATs) are imported via their peroxisomal targeting
sequence (PTS), either a PTS1 or PTS2. However, a number of studies demonstrate that
some MATs that lack a recognizable PTS sequence can also be imported into
peroxisomes. It is proposed that these proteins can bind to other MATs with a defined
PTS signal, or that they contain an as yet unidentified PTS required for targeting. Hence,
the use of bioinformatics to identify PTS1/PTS2 signals in putative MATs is not
sufficient to obtain an overview of which matrix proteins target to peroxisomes and
instead top down techniques such as mass spectrometry based organellar proteomics are
required. Furthermore, studies that aim to define how MATs that lack a PTS target to
Introduction ONE
35
peroxisomes will undoubtedly result in the identification of additional peroxisomally
localised metabolic pathways which, when taken together with mass spec based
approaches, will increase our understanding of the role of peroxisomes in cellular
metabolism.
Peroxisomal protein import is vital for peroxisomal function and likewise the
removal and degradation of certain peroxisomal proteins will also likely impact on
peroxisome biology. Unlike the degradation of membrane proteins from other organelles,
little is known about the turnover of PMPs. The degradation of specific PMPs via the
ubiquitin-proteasome system (UPS) rather than the selective autophagy of peroxisome
(pexophagy) provides the possibility that PMPs can be selectively degraded without
interfering other metabolism pathways. To date Pex3p in H. polymorpha and Pex13p in
plants are the only PMPs known to be targeted for degradation via the UPS (Bellu et al,
2002; Pan et al, 2016; Williams & van der Klei, 2013a) and the question remains which
other PMPs are degraded via the UPS and why? Furthermore, the mechanisms of Pex3p
and Pex13p degradation appear to differ quite dramatically, which raises the question
whether different pathways (and hence different ubiquitin-conjugating enzymes and E3
ligases) exits to target PMPs for UPS-mediated degradation. TRIM37, a peroxisomally
localised E3 ligase in mammals, ubiquitinates Pex5p to protect it from proteasomal
degradation (Wang et al, 2017). It will be interesting to see whether TRIM37
ubiquitinates other peroxisomal proteins. Finally, how the removal of Pex3p and Pex13p
(as well as other putative PMPs) from the peroxisomal membrane is achieved is
currently unknown. In the case of H. polymorpha Pex3p, the AAA-ATPase Pex1p was
not required, suggesting the involvement of another AAA-ATPase in dissociating Pex3p
from the membrane.
9. Aim and outline of this thesis
Peroxisomes are single membrane bound organelles found in virtually all eukaryotic
cells. They are involved in multiple metabolic functions including the decomposition of
reactive oxygen species and the oxidation of fatty acids, but many more peroxisomal
functions are known. Peroxisomal functions depends on the matrix and membrane
proteins present in peroxisomes and regulating which proteins are present in a given
peroxisome at a given time allows peroxisome function to be finely tuned.
Peroxisomes lack DNA, which means that they import all the peroxisomal matrix
and membrane proteins required for function. Hence, the import of peroxisomal proteins
plays an important role in defining peroxisome function. Likewise, the removal and
degradation of peroxisomal proteins can also be expected to impact on peroxisomal
ONE Introduction
36
function yet to date little is known on how or why peroxisomal protein degradation
occurs.
The aim of the research presented in this thesis is to provide the first insights into
peroxisomal membrane protein (PMP) degradation. The presence of an intricate
ubiquitination machinery on the peroxisomal membrane suggests that this machinery
targets PMPs for ubiquitination and degradation, as do similar machineries on other
organelles, yet to date the only PMP substrate of this machinery is Pex3p in the yeast H.
polymorpha. The identification of additional substrates of the peroxisomal
ubiquitination machinery will therefore allow us to better understand the role of this
machinery in peroxisome function. Likewise, since protein degradation can occur for
different reasons, understanding why PMPs are targeted for degradation will also
provide information on the importance of PMP degradation in peroxisome function. To
address these issues, the research presented here utilizes a multi-disciplinary approach to
investigate some of the underlying mechanisms and cellular functions of PMP
degradation in yeast.
In Chapter one, we presented an overview of processes that regulate peroxisome
function. In addition, the Ubiquitin proteasome system is discussed, as was as how
organelle membrane protein degradation is regulated and facilitated.
Previous findings suggested that the peroxisomal ubiquitination machinery is
involved in the degradation of the PMP Pex3p degradation in the yeast H. polymorpha.
In Chapter two we aimed to identify additional substrates of this machinery in PMP
degradation using H. polymorpha as model organism. Our data demonstrate that levels
of the PMP Pex13p build up in cells lacking members of the peroxisomal ubiquitination
machinery and also establish that Pex13p undergoes rapid degradation in wild type cells.
Furthermore, we show that Pex13p is ubiquitinated in wild type cells and also establish
that Pex13p ubiquitination is reduced in cells lacking a functional peroxisomal E3 ligase
complex. Finally, deletion of PEX2 causes Pex13p to build up at the peroxisomal
membrane. Taken together, our data suggest that Pex13p degradation regulates
peroxisomal matrix protein import. Furthermore, this study provides further evidence
that the role of the peroxisomal ubiquitination machinery in peroxisome biology goes
much deeper than receptor recycling alone.
Pex13p in the yeast H. polymorpha undergoes rapid degradation in a process that
requires the peroxisomal E3 ligase Pex2p. However, the underlying reason why Pex13p
undergoes degradations remained unknown. In Chapter three we have investigated the
degradation of H. polymorpha Pex13p further, aiming to understand the underlying
reasons why Pex13p undergoes rapid degradation. Our data indicate that
Introduction ONE
37
Pex2p-dependent turnover of Pex13p also occurs under peroxisome non-inducing
condition, demonstrating that Pex13p degradation is a general and not a media-specific
event. In addition, our studies indicate that blocking Pex5p recycling leads to increased
Pex13p levels, suggesting that Pex5p recycling is functionally linked to Pex13p turnover.
Furthermore, we identify a mutant version of Pex13p that is inhibited in degradation and
we also establish that inhibiting Pex13p degradation can impact negatively on cell
growth on methanol-containing media. Based on these results, we outline possible
functions of Pex13p degradation in relation to the import of peroxisomal matrix
proteins.
The link between Pex13p degradation and peroxisomal matrix protein import
identified in Chapter three suggests that this degradation event may be a general trait for
peroxisomes. Hence, we aimed to investigate whether Pex13p degradation is a
conserved process across species, choosing the yeast S. cerevisiae as model organism.
Furthermore, we aimed to utilise the high-throughput screening techniques available for
this organism to identify additional factors that are required for Pex13p degradation. In
Chapter four, we demonstrate that UPS-mediated Pex13p degradation also occurs in
the yeast S. cerevisiae, likely via similar mechanisms to that in H. polymorpha.
Furthermore, inactivation of the ATPase Cdc48p, which plays a role in degrading
mitochondrial and ER membrane proteins, does not result in stabilization of Pex13p in
vivo, establishing that Pex13p degradation probably occurs via a different mechanism to
that of other organellar membrane proteins. Additionally, we utilize a tandem fluorescent
protein timer approach to identify which additional factors are involved in Pex13p
degradation, establishing that cytosolic E2 and E3 enzymes may also play a role in
Pex13p turnover. Together, these data provide further evidence that Pex13p degradation
is a conserved process while also uncovering novel components of the UPS that play a
role in Pex13p degradation. We discuss the implications of our findings.
The proteins that are present in peroxisomes determine peroxisomal function.
These are the matrix involved in the different peroxisomally localised pathways or the
membrane proteins that transport metabolites or proteins across the peroxisomal
membrane. Additional peroxisomal proteins are involved in organelle biogenesis and
dynamics. Therefore, obtaining a complete overview of the proteins present in
peroxisomes at a given time or under a given growth condition provides invaluable
insights into peroxisome function. In Chapter five we provide an overview of how mass
spectrometry based proteomics studies have provided valuable new and novel insights
into peroxisomal function and we outline how innovative new techniques and
approaches may lead to new discoveries in the future.
38
2
Chapter 2
Insights into the role of the peroxisomal ubiquitination machinery in Pex13p
degradation in the yeast Hansenula polymorpha
Xin Chen, Srishti Devarajan, Natasha Danda and Chris Williams
This chapter has been published: (Featured Article)
Chen, X., Devarajan, S., Danda, N., & Williams, C. (2018). Insights into the role of the
peroxisomal ubiquitination machinery in Pex13p degradation in the yeast Hansenula
polymorpha. Journal of molecular biology, 430(11), 1545-1558.
Author contributions
CW conceived and supervised the project. CW, SD, ND and XC designed the
experiments. XC, SD, ND and CW analysed the data. XC performed biochemical and
FM experiments, with support from SD and ND. All authors discussed the results. XC
and CW wrote the manuscript, with contributions from all authors.
TWO Pex13p degradation in H. polymorpha
40
Insights into the role of the peroxisomal ubiquitination machinery in Pex13p
degradation in the yeast Hansenula polymorpha
Xin Chen1, Srishti Devarajan
1, Natasha Danda
1,2 and Chris Williams
1,*
1Molecular Cell Biology, Groningen Biomolecular Sciences and Biotechnology Institute,
University of Groningen, 9747AG, the Netherlands 2Current address: Institut du Cerveau et de la Moelle épinière (ICM), Hôpital
Pitié-Salpêtrière, 47 bd de l'Hôpital, 75013 Paris, France
*Corresponding author ([email protected])
Abstract
The import of matrix proteins into peroxisomes in yeast requires the action of the
ubiquitin conjugating enzyme Pex4p and a complex consisting of the ubiquitin E3
ligases Pex2p, Pex10p and Pex12p. Together, this peroxisomal ubiquitination machinery
is thought to ubiquitinate the cycling receptor protein Pex5p and members of the Pex20p
family of co-receptors, a modification that is required for receptor recycling. However,
recent reports have demonstrated that this machinery plays a role in additional
peroxisome-associated processes. Hence, our understanding of the function of these
proteins in peroxisome biology is still incomplete. Here, we identify a role for the
peroxisomal ubiquitination machinery in the degradation of the peroxisomal membrane
protein Pex13p. Our data demonstrate that Pex13p levels build up in cells lacking
members of this machinery and also establish that Pex13p undergoes rapid degradation
in wild type cells. Furthermore, we show that Pex13p is ubiquitinated in wild type cells
and also establish that Pex13p ubiquitination is reduced in cells lacking a functional
peroxisomal E3 ligase complex. Finally, deletion of PEX2 causes Pex13p to build up at
the peroxisomal membrane. Taken together, our data provide further evidence that the
role of the peroxisomal ubiquitination machinery in peroxisome biology goes much
deeper than receptor recycling alone.
Keywords: Peroxisome/protein degradation/ubiquitin proteasome
system/PMP/peroxisomal membrane protein
Pex13p degradation in H. polymorpha TWO
41
Introduction
Peroxisomes are highly versatile eukaryotic organelles that play a vital role in regulating
cellular metabolism, providing compartments where metabolic pathways can be
contained and controlled. Their versatility is demonstrated by the wide range of
metabolic pathways contained in peroxisomes. Some well-known peroxisomal processes
include the oxidation of fatty acids and the biosynthesis of plasmalogens and penicillin,
but many more exist (Gabaldon, 2010). Their importance in cell vitality is underscored
by a number of inherited developmental brain disorders caused by defects in peroxisome
biogenesis (Walker et al, 2002). Peroxisomes require protein import systems to obtain
both peroxisomal membrane (PMP) and matrix proteins, via the use of peroxisomal
targeting signals (PTS) in the cargo protein. The mechanisms of PMP import are not
well understood, although important roles for the PMP Pex3p and the cytosolic receptor
protein Pex19p have been demonstrated (Ferreira et al, 2015; Jung & Grune, 2013). In
contrast, our understanding of the mechanisms that underlie matrix protein import is
much more developed (Baker et al, 2016). Matrix proteins containing a C-terminal PTS1
can be recognized by the cytosolic receptor Pex5p while matrix proteins with an
N-terminal PTS2 are recognized by Pex7p (Lazarow, 2006; Williams & Stanley, 2010).
In yeasts, Pex7p requires members of the Pex20p family of co-receptor proteins to
facilitate import, whereas this function is fulfilled by an isoform of Pex5p in higher
eukaryotes (Schliebs & Kunau, 2006). Pex5p shuttles between the cytosol and
peroxisomal membrane during the transport of PTS1-cargo proteins. The cargo-Pex5p
complex, which forms in the cytosol, travels to the peroxisomal membrane, where it
contacts the docking complex consisting of the PMPs Pex13p and Pex14p. After
translocation of the cargo to the peroxisomal matrix in a process involving Pex8p, Pex5p
is ubiquitinated, which facilitates its removal from the peroxisomal membrane (for a
review on matrix protein import, see (Baker et al, 2016)).
Ubiquitination is a posttranslational modification that requires the activity of a
three-step enzyme cascade (Komander & Rape, 2012). The ubiquitin-activating enzyme
(E1) activates the small protein ubiquitin (Ub) via ATP hydrolysis and transfers it to the
active site Cysteine of an ubiquitin-conjugation enzyme (E2). The final step requires the
activity of an ubiquitin ligase (E3). Two classes of E3s exist. Members of the HECT
class, much like E2s, accept Ub onto an active site Cysteine and then transfer Ub to a
substrate, whereas RING E3 ligases act as bridge between E2 and substrate, positioning
the E2 active site in close proximity to the modification site in the substrate, allowing
Ub transfer to occur .
Two distinct types of Pex5p ubiquitination have been reported.
TWO Pex13p degradation in H. polymorpha
42
Mono-ubiquitination of Pex5p on a conserved Cysteine residue in its N-terminal region
by the E2 Pex4p allows Pex5p to recycle to the cytosol, ready to take part in another
import round (Grou et al, 2009; Platta et al, 2007; Williams et al, 2007).
Poly-ubiquitination of Pex5p on Lysine residues by the E2 Ubc4p, on the other hand,
targets Pex5p for degradation via the proteasome (Kiel et al, 2005a; Platta et al, 2004).
For both types of Pex5p ubiquitination, a complex consisting of three peroxisomal
RING E3s (Pex2p, Pex10p and Pex12p) is required (El Magraoui et al, 2014; Williams
et al, 2008) while extraction of ubiquitinated Pex5p from the membrane depends on a
complex of the AAA-ATPase proteins Pex1p and Pex6p (Platta et al, 2008). Pex20p
family members can also undergo ubiquitination, either for recycling or degradation, in
a similar fashion as mentioned for Pex5p (Leon et al, 2006).
It is evident that the peroxisomal ubiquitination machinery (Pex4p, Pex2p, Pex10p
and Pex12p) is important for peroxisome function because of its role in receptor
ubiquitination. However, recent reports link this machinery to the ubiquitination and/or
degradation of additional peroxisomal proteins. For example, the PMP Pex3p from the
yeast Hansenula polymorpha is ubiquitinated and degraded by the proteasome when
cells are shifted from methanol to glucose containing media (Williams & van der Klei,
2013b). Pex3p degradation, which is inhibited in pex2Δ and pex10Δ cells, initiates the
autophagic degradation of peroxisomes via pexophagy (Bellu et al, 2002). Pex2p is
implicated in PMP70 ubiquitination in mammalian cells, which is also linked to
pexophagy (Knoblach et al, 2013), while Pex4p is involved in the degradation of the
PTS2 co/receptor protein Pex18p in Saccharomyces cerevisiae (Purdue & Lazarow,
2001). These reports demonstrate that the list of substrates targeted by the peroxisomal
ubiquitination machinery is likely to be far from complete.
In this manuscript, we have investigated the role of the peroxisomal ubiquitination
machinery in the degradation of the PMP Pex13p. Cells deleted for components of the
peroxisomal ubiquitination machinery display enhanced Pex13p levels while we also
demonstrate that Pex13p is degraded in wild type (WT) cells. Furthermore, we show
that Pex13p is ubiquitinated in WT cells and that Pex13p ubiquitination is inhibited in
cells lacking a functional peroxisomal E3 ligase complex. Finally, we demonstrate that
deletion of PEX2 causes Pex13p to build up on the peroxisomal membrane. Taken
together, our data provide further evidence to support the suggestion that the role of the
peroxisomal ubiquitination machinery goes much deeper than receptor ubiquitination
alone.
Pex13p degradation in H. polymorpha TWO
43
Results
Pex13p levels are increased in cells deleted for components of the peroxisome
ubiquitination machinery
While a role for the peroxisome ubiquitination machinery in receptor ubiquitination is
well established, recent reports strongly suggest that this machinery targets additional
peroxisomal proteins. Therefore, we set out to identify potential new substrates of this
machinery in the yeast H. polymorpha and were particularly interested in which PMPs
may be targeted, since little is known about PMP degradation (Williams, 2014).
We reasoned that PMPs targeted for degradation by the peroxisomal ubiquitination
machinery may display increased levels in cells deleted for components of this
machinery. Therefore, we assessed the levels of a selection of PMPs in cells deleted for
PEX2, PEX4, PEX10 or PEX12 grown on methanol/ glycerol containing media, which
induces peroxisome proliferation. These PMPs, which are involved in different
peroxisomal functions, included Pex13p and Pex14p (both involved in matrix protein
import (Azevedo & Schliebs, 2006; Williams & Distel, 2006)), Pex3p (involved in PMP
import (Tomisugi et al, 2000)) and Pex11p (involved in peroxisomal fission
(Maupin-Furlow et al, 2005)). We observed that Pex13p levels were increased in all the
tested strains compared to WT cells (Figure 1A) and Pex13p levels appeared particularly
enhanced in cells deleted for PEX2, PEX10 or PEX12. Similarly, cells expressing the
K48R mutant form of Ub also displayed enhanced Pex13p levels, although not to the
same extent as those deleted for one of the peroxisomal E3 ligases (Figure 1A).
Ub-K48R inhibits proteasomal mediated degradation by blocking Ub chain formation on
substrates (Thrower et al, 2000), suggesting a link between Pex13p levels and the
ubiquitin-proteasome system (UPS). An increase in Pex3p and Pex14p levels in these
deletion strains was also observed (Figure 1A). A role for the peroxisomal ubiquitination
machinery in Pex3p degradation has already been proposed (Williams & van der Klei,
2013b) although Pex3p degradation was shown to occur under different growth
conditions than those used here. Pex11p levels appeared largely unaffected in the
deletion strains (Figure 1A).
TWO Pex13p degradation in H. polymorpha
44
Figure 1. H. polymorpha Pex13p levels are elevated in cells deleted for components
of the peroxisomal ubiquitination machinery
A WT cells, together with pex2Δ, pex10Δ, pex12Δ and pex4Δ cells and WT cells producing
Pex13p degradation in H. polymorpha TWO
45
Ub-K48R grown for 16 hrs on methanol/glycerol media were lysed and samples were
subjected to SDS-PAGE and immunoblotting using antibodies directed against Pex3p,
Pex13p, Pex14p, Pex11p and Pyc. * Denotes anti-Pex13p cross reactive species. L.E.
stands for longer exposure.
B Bar chart displaying Pex13p, Pex14p and Pex11p levels in WT, pex2Δ and pex4Δ cells.
Values were derived from quantifying western blots of samples prepared as in A. Protein
levels were normalized to Pyc (loading control) and plotted against the levels in WT
cells (set to 1). Values represent the mean ± standard deviation of three independent
experiments. Asterisks denote statistically significant increases in protein levels
compared to those in WT samples (*P < 0.05, **P < 0.01, ***P < 0.001).
C Representative western blots of Pex13p, Pex14p, Pex11p and Pyc levels in WT, pex13Δ
and aoxΔ cells grown and treated as in A. * Denotes anti-Pex13p cross reactive species.
The right panel displays the quantification of Pex13p, Pex14p and Pex11p levels,
normalized to the loading control Pyc. Protein levels in WT cells were set to 1. Values
represent the mean ± SD of three independent experiments.
D WT and mutant cells expressing mGFP under control of the PEX13 promoter (PPEX13)
were grown for 16 hrs on methanol/glycerol containing media, lysed and samples were
probed with SDS-PAGE and immunoblotting using antibodies against mGFP and Pyc.
E TCA lysates of WT cells, WT cells producing Ub-K48R and atg1 cells grown on
methanol/glycerol media for 16 hrs were subjected to SDS-PAGE, immunoblotting and
probed with antibodies directed against Pex11p, Pex13p, Pex14p and Pyc. * Denotes
anti-Pex13p cross reactive species.
To gain insight into the extent to which Pex13p levels were increased in these
deletion strains compared to WT cells, we performed quantitative western blotting,
assessing the fold increase in Pex13p levels in pex4Δ and pex2Δ cells (Figure 1B).
Deletion of either PEX2, PEX10 or PEX12 results in inactivation of the entire E3 ligase
complex (Agne et al, 2003), hence our choice to assess Pex13p levels in pex2Δ cells
only. Pex13p levels increased around 4fold in pex4Δ cells and around 12fold in pex2Δ
cells, compared to WT. Quantification of our western blots also confirmed that Pex14p
levels were increased in pex2Δ or pex4Δ cells compared to WT cells, although to a much
lower extent than for Pex13p (Figure 1B). As already suggested by Figure 1A, Pex11p
levels were not significantly affected by deletion of PEX2 or PEX4 (Figure 1B).
Because of the dramatic effect on Pex13p levels caused by these deletions, we chose to
investigate Pex13p further.
TWO Pex13p degradation in H. polymorpha
46
Deletion of PEX2, PEX4, PEX10 or PEX12 inhibits the import of matrix proteins
into peroxisomes (Baker et al, 2016). Since the oxidation of methanol occurs inside
peroxisomes and targeting the enzymes required for methanol metabolism to the cytosol
inhibits cells in their ability to grow on methanol, strains where matrix protein import is
inhibited cannot be grown on methanol (Cregg et al, 1990). Therefore, we investigated
whether the increased Pex13p levels in our deletion strains stem from an inability of
these strains to grow on methanol/ glycerol containing media. We compared the levels of
Pex13p in WT cells against cells deleted for alcohol oxidase (AOX). AOX is required
for methanol oxidation and cells deleted for AOX cannot be grown on methanol
(Bridges et al, 2016). We observed no increase in Pex13p levels in aoxΔ cells (Figure
1C), indicating that the increased Pex13p levels in cells deleted for PEX2, PEX4,
PEX10 or PEX12 are not caused by an inability of these cells to grow on methanol
containing media.
Next, to verify that the increased levels of Pex13p in these mutant strains were not
a result of increased Pex13p expression, we placed mGFP under control of the PEX13
promoter and assessed mGFP levels in our deletion and Ub-K48R mutant strains. The
level of mGFP in all mutants was comparable to that in WT cells (Figure 1D). These
data demonstrate that PEX13 expression is not up-regulated in these strains.
The major protein degradation pathway in eukaryotic cells is the UPS (Rowland et
al, 2014). However, certain proteins can be degraded via autophagy (Maupin-Furlow et
al, 2003) and although these two pathways are separate entities, crosstalk between the
two pathways is well established (Liu et al, 2002). For example, ubiquitination of
PMP70 by Pex2p initiates pexophagy in mammalian cells (Knoblach et al, 2013) while
we previously demonstrated that Pex10p plays a role in degradation of Pex3p, which in
turn initiates pexophagy in H. polymorpha (Williams & van der Klei, 2013b). Hence, we
considered the possibility that the effect on Pex13p levels in our deletion strains may
result as a consequence of disturbances to pexophagy. To investigate this, we assessed
the levels of Pex13p in an atg1Δ strain, in which pexophagy is inhibited (Knoops et al,
2014). We did not observe an increase in Pex13p levels in atg1Δ cells (Figure 1E),
demonstrating that increased Pex13p levels do not stem from inhibiting pexophagy. It
suggests that increased Pex13p levels stem from a block in UPS-dependent Pex13p
degradation. Together, our data suggest that Pex13p is a potential substrate of the
peroxisomal ubiquitination machinery.
Pex13p degradation in H. polymorpha TWO
47
Figure 2. H. polymorpha Pex13p is actively degraded in WT cells.
A WT cells were grown on methanol/glycerol media for 12 hrs and then treated with DMSO
(Ctrl) or Cycloheximide (CHX). TCA samples were taken at the indicated time (hrs) after
DMSO/CHX addition and probed by SDS-PAGE and immunoblotting with antibodies
against Pex13p, Pex14p, Pex11p and Pyc. * Denotes anti-Pex13p cross reactive species.
B Quantification of Pex13p, Pex14p and Pex11p levels in WT cells treated with DMSO
(Ctrl) or Cycloheximide (CHX). Protein levels were normalized to Pyc. Protein levels at
T0 were set to 1. Values represent the mean ± SD of three independent experiments.
C Representative western blots of WT cells expressing Pex13-mGFP grown and treated as
in A. Western blots were probed using antibodies against Pex14p, Pex11p, Pyc and
mGFP.
D Quantification of protein levels in WT cells expressing Pex13-mGFP after DMSO/CHX
addition. The data were generated as in B.
Pex13p is degraded in WT cells and Pex13p degradation requires a functional
peroxisomal E3 ligase complex
Since deleting components of the peroxisomal ubiquitination machinery seem to block
Pex13p degradation (Figure 1), our next step was to investigate whether Pex13p is
actively degraded in WT cells. To achieve this, we assessed the stability of Pex13p in
WT cells treated with the protein synthesis inhibitor cycloheximide (CHX). We
observed rapid decrease of Pex13p levels after CHX treatment (Figure 2A and B) while
TWO Pex13p degradation in H. polymorpha
48
similar behaviour was evident with Pex13-mGFP (Figure 2C and D), establishing that
Pex13p is actively degraded in WT cells. The Pex13-mGFP used here could not only
give similar degradation behavior and clearer signal, but important for the later
fluorescence microscopy (Figure 6). In contrast, Pex13-mGFP turnover was reduced in
cells expressing Ub-K48R (Figure 3A and B) and in cells deleted for PEX2 (Figure 3C
and D), supporting our suggestion that Pex13p degradation is inhibited in cells lacking a
functional peroxisomal E3 ligase complex, as well as in cells expressing Ub-K48R
(Figure 1).
We observed that the levels of Pex14p and Pex11p in our CHX experiments
decreased over time, although at a lower rate than Pex13p (Figure 2A-D). Also, Pex11p
and Pex14p appeared stable in cells expressing Ub-K48R (Figure 3A and B) and in
pex2Δ cells (Figure 3C and D). One possible way to interpret these data is that both
Pex11p and Pex14p may also be degraded in a process that requires the peroxisomal E3
ligase complex and Ub, although further study will be required to determine whether
this is indeed the case. Nevertheless, our data strongly suggest that Pex13p is actively
degraded in a process that requires Ub and the peroxisomal E3 ligase complex.
Figure 3. Pex13p degradation is inhibited in pex2Δ or Ub-K48R cells
A Ub-K48R cells expressing Pex13-mGFP were grown on methanol/glycerol media for 12
hrs and treated with DMSO (Ctrl) or Cycloheximide (CHX). TCA samples were taken at
the indicated time (hrs) after DMSO/CHX addition and probed by SDS-PAGE and
immunoblotting with antibodies against mGFP, Pex14p, Pex11p and Pyc.
Pex13p degradation in H. polymorpha TWO
49
B Quantification of Pex13-mGFP, Pex14p and Pex11p levels in Ub-K48R cells expressing
Pex13-mGFP. Protein levels were normalized to the loading control Pyc. Protein levels
at T0 were set to 1. Values represent the mean ± SD of three independent experiments.
C Representative western blots of pex2Δ cells expressing Pex13-mGFP derived from cells
grown and treated as in A. Samples were probed with SDS-PAGE and immunoblotting
with antibodies against mGFP, Pex11p and Pyc.
D Quantification of protein levels in pex2Δ cells expressing Pex13-mGFP. Protein levels
were normalized to Pyc. Protein levels at T0 were set to 1. Values represent the mean ±
SD of three independent experiments.
Pex13p is ubiquitinated in WT cells while Pex13p ubiquitination is reduced in pex2Δ
cells
To investigate more directly the role of Ub and the peroxisomal E3 ligase complex in
Pex13p degradation, we assessed whether Pex13p is ubiquitinated. To achieve this, we
introduced a C-terminal His6 tagged form of Pex13p into WT and pex2Δ cells and
performed pull-down assays (Figure 4). Cells also co-produced a Myc tagged form of
Ub (Myc-Ub), to aid detection of ubiquitinated proteins. A ladder of Myc-Ub
Pex13-His6 was detected in elution fractions isolated from WT cells co-expressing
Pex13-His6 and Myc-Ub (Figure 4B, lane 4). This ladder was severely reduced in
elution fractions isolated from pex2Δ cells co-expressing Pex13-His6 and Myc-Ub
(Figure 4B, lane 3), providing direct evidence that Pex13p is ubiquitinated in WT cells
and also showing that Pex13p ubiquitination requires the peroxisomal E3 ligase
complex.
TWO Pex13p degradation in H. polymorpha
50
Figure 4. Pex13p is ubiquitinated in WT cells while Pex13p ubiquitination is
reduced in pex2Δ cells.
pex2/Myc-Ub, pex2/Pex13-His, pex2/Pex13-His/Myc-Ub and Pex13-His/Myc-Ub cells were
grown on methanol/glycerol media for 12 hrs and Pex13-His was purified under denaturing
conditions using Ni-NTA resin. Load (A) and elution (B) fractions were subjected to
SDS-PAGE and immunoblotting with antibodies raised against the Myc-tag (upper panels)
or the His tag (lower panels).
Pex13p degradation in H. polymorpha TWO
51
Figure 5. Pex13p levels are elevated in pex5Δ, pex14Δ and pex8Δ cells.
A Representative western blots of samples derived from WT and mutant cells grown for 16
hrs on methanol/glycerol media. Blots were probed with antibodies directed against
Pex13p, Pex14p, Pex11p and Pyc. * Denotes anti-Pex13p cross reactive species.
B Lysates from WT, pex4Δ and pex8Δ cells (grown as in A) were subjected to SDS-PAGE
and immunoblotting using antibodies against Pex13p, Pex14p, Pex11p and Pyc. *
Denotes anti-Pex13p cross reactive species.
C Quantification of protein levels in WT and mutant cells, normalized to the loading
control Pyc. Protein levels in WT cells were set to 1. Values represent the mean ± SD of
three independent experiments. Asterisks denote statistically significant increases in
protein levels compared to those in WT samples (*P < 0.05, **P < 0.01, ***P < 0.001).
TWO Pex13p degradation in H. polymorpha
52
Pex5p, Pex14p and Pex8p play a role in Pex13p degradation
Next we sought to identify whether additional proteins are required for Pex13p
degradation and focussed on proteins that were shown to interact with Pex13p in other
organisms. These included the PTS1 receptor protein Pex5p (Douangamath et al, 2002),
the docking factor Pex14p (Pires et al, 2003), the PTS2 receptor Pex7p (Stein et al, 2002)
and its accompanying co-receptor protein Pex20p (Stein et al, 2002) and the
cargo-dissociation factor Pex8p (Jung et al, 2009). Deletion of genes that encode for
proteins specifically involved in PTS2 protein import did not impact on Pex13p
degradation (Figure 5A and C) whereas Pex13p levels were increased around 3fold in
cells deleted for PEX5 and around 6fold in cells deleted for PEX14 (Figure 5A-C).
Strikingly, PEX8 deletion resulted in a strong inhibition of Pex13p degradation, at a
level comparable with that observed for pex2Δ cells (Figure 5B and C). Pex14p levels
were also increased in cells deleted for PEX8, although to a much lower extent, similar
to in cells deleted for PEX2 (Figure 1B and 5C). Deletion of PEX5, PEX8 or PEX14 did
not affect PEX13 promotor activity (Figure 1D), indicating that the increased levels of
Pex13p indeed stem from inhibited protein degradation. We also observed what
appeared to be modified forms of Pex13p in samples derived from pex5Δ, pex14Δ,
pex2Δ or pex8Δ cells (denoted with a # in Figure 5A and B). We consider it highly
unlikely that these represent ubiquitinated forms of Pex13p, because deletion of PEX2
inhibits Pex13p ubiquitination (Figure 4), which leaves us to conclude that they
represent another modified form of Pex13p that becomes visible because Pex13p levels
are increased in these deletion strains. We can only speculate as to which modification
this could represent but since phosphorylated Pex13p peptides have been found in
mammalian cells (Schluter, 2006), it may represent phosphorylated Pex13p.
Taken together, these observations demonstrate that additional factors are likely to
play a role in Pex13p degradation.
Pex13-mGFP builds up at the peroxisomal membrane in pex2Δ cells
Our data could suggest that Pex13p is ubiquitinated by the peroxisomal ubiquitination
machinery for proteasomal mediated degradation. Since this machinery is present at the
peroxisomal membrane and proteasomes are mostly cytosolic (Lee et al, 2017), we
considered it likely that Pex13p would build up on the peroxisomal membrane when its
degradation is inhibited. To investigate this further, we compared the behaviour of
Pex13-mGFP in WT and pex2Δ cells using fluorescence microscopy (FM). Cells also
co-produced Pex14-mKate2, to mark peroxisomes. As expected, both Pex13-mGFP and
Pex14-mKate2 co-localised in WT cells (Figure 6A and B). In Figure 6A, fluorescence
Pex13p degradation in H. polymorpha TWO
53
images were processed with each optimal settings to clearly show signals, while in
Figure 6B, images were processed with a common setting to reflect the difference of
fluorescence intensities in two strains. pex2Δ cells lack functional peroxisomes, because
Pex2p is required for matrix protein import (Koek et al, 2007). Instead, pex2Δ cells
contain peroxisome “ghosts”, which are small peroxisomal membrane structures that
contain most PMPs but very few matrix proteins (Koek et al, 2007). Pex13-mGFP
co-localized with Pex14-mKate2 in peroxisomal ghosts in pex2Δ cells (Figure 6 A and
B). As expected, Pex13-mGFP was present at higher levels in pex2Δ cells, as can be
seen from the increased GFP signal in cells (Figure 6C), as well as protein levels (Figure
6D) in pex2Δ cells compared to WT cells. Taken together, these results indicate that
Pex13-mGFP builds up on the peroxisomal membrane in the absence of a functional
peroxisomal E3 ligase complex.
Figure 6. Pex13-mGFP accumulates on the peroxisomal membrane in pex2Δ cells.
A WT and pex2Δ cells producing Pex13-mGFP and Pex14-mKate2 were grown on
methanol/glycerol media to an OD600 of 1.0 and fluorescence microscopy images were
TWO Pex13p degradation in H. polymorpha
54
taken. Images of Pex13-mGFP were processed using ImageJ with optimal settings to
show signals in WT and pex2Δ. Pex14-mKate2 was used as peroxisomal membrane
marker. The following settings were used: for WT cells mGFP (255, 2500) and mKate2
(219, 3000); for pex2 cells mGFP (255, 7000) and mKate2 (219, 4700). Scale bar: 5μm.
B Fluorescence images of Pex13-mGFP in WT or pex2Δ shown in (A) were processed
using ImageJ with the same settings: mGFP (255, 5000), mKate2 (219, 4000). Scale bar:
5μm.
C Box plot showing quantification of mGFP and mKate2 fluorescence intensity at the
peroxisomal membrane in WT and pex2Δ cells producing Pex13-mGFP and
Pex14-mKate2. Fluorescence intensities (auxiliary units) were measured using ImageJ.
The box represents values from the 25 percentile to the 75 percentile; the horizontal line
through the box represents the median value. Whiskers indicate maximum and minimum
values. Pex13-mGFP and Pex14-mKate2 measurements were taken as described in the
Materials and Methods section.
D The intensity ratio of mGFP/ mKate calculated based on the same cells from Fig-6C.
The maximum intensity of Pex13-mGFP was divided by the corresponding maximum
intensity of Pex14-mKate2 in each cell. The dataset subjected to the two-tail t-test
resulting P-value 0.001 .
E WT and pex2Δ cells producing Pex13-mGFP grown on methanol/glycerol media and
TCA samples were taken when the cultures reached an OD600 of 1.0. Samples were
subjected to SDS-PAGE and immunoblotting using antibodies against mGFP and Pyc.
Discussion
The molecular function of the peroxisomal ubiquitination machinery was long thought
to be restricted to cycling receptor ubiquitination. However, several recent reports have
identified additional roles for this machinery in peroxisome biology. Here, we present
data that suggest a role for the E2 Pex4p and the RING E3 ligases Pex2p, Pex10p and
Pex12p in the degradation of Pex13p while we also provide evidence that Pex13p is
ubiquitinated in a manner that requires a functional peroxisomal E3 ligase complex.
Following this line of reasoning, our data suggest a model where Pex13p is
ubiquitinated by Pex4p and the peroxisomal E3 ligase complex to target Pex13p for
proteasomal mediated degradation. While this model is an attractive proposal, it remains
hypothetical at the current time because we have not shown that the peroxisomal
ubiquitination machinery is directly involved in Pex13p ubiquitination. Such evidence
will likely come from the use of assays that reconstitute the ubiquitination of Pex13p in
Pex13p degradation in H. polymorpha TWO
55
vitro. Nevertheless our data, when coupled together with the observations that Pex5p
(Kiel et al, 2005a; Platta et al, 2004), members of the Pex20p family (Liu & Subramani,
2013; Purdue & Lazarow, 2001) and Pex7p (Hagstrom et al, 2014) can all be
ubiquitinated for proteasomal mediated degradation, indicate that the UPS is involved in
targeting a range of peroxisomal proteins for degradation, suggesting a determining role
for the UPS in regulating peroxisome function.
This leads to the question why is Pex13p targeted for degradation? Currently, it is
only possible to speculate on this. Since Pex13p is essential for peroxisomal matrix
protein import (Williams & Distel, 2006), degradation of Pex13p would likely inhibit
the import process. In this light, an interesting comparison can be drawn with recent
work on Arabidopsis Pex13p (Helle et al, 2013). Here, the authors reported that
Arabidopsis Pex13p can be degraded by the RING E3 Ligase SP1 in vivo. SP1 also
facilitates the ubiquitination and degradation of TOC (translocon at the outer envelope
of chloroplasts) complexes, controlling the import of proteins into chloroplasts
(Knoblach & Rachubinski, 2015). While a role for SP1 in peroxisomes remains
controversial (Huh, 2003; Rabellino et al, 2017), our data would fit a model similar to
the one proposed by Pan et al, which suggests that Pex13p degradation negatively
regulates peroxisomal matrix protein import by downregulating import complexes on
the peroxisomal membrane (Helle et al, 2013). Alternatively, the peroxisomal
ubiquitination machinery may target damaged or incorrectly folded Pex13p for
degradation, in a similar way to the endoplasmic reticulum associated degradation
(ERAD) pathway (Smith et al, 2011). Either way, we predict that Pex13p degradation
will impact on peroxisomal matrix protein import, making it an interesting topic for
further study.
Our data also indicate a role for the cycling receptor Pex5p, the docking protein
Pex14p and the intraperoxisomal protein Pex8p in Pex13p degradation. How these
proteins may be involved in Pex13p degradation is unclear at the current time, although
the involvement of Pex5p and Pex14p could suggest that Pex13p degradation is linked
to PTS1 protein import. Likewise, the effect of deleting PEX8 on Pex13p degradation
could also suggest a link to PTS1 protein import. However, this may stem from a
different reason. Pex13p binds to Pex8p and this interaction was proposed to allow the
docking complex, consisting of Pex13p, Pex14p and Pex17p, to contact the E3 ligase
complex consisting of Pex2p, Pex10p and Pex12p (Agne et al, 2003). Such a model
would suggest that Pex13p and the E3 ligase complex are unable to associate in cells
deleted for PEX8, which may result in a block to Pex13p ubiquitination and hence,
degradation. The increase in Pex13p levels in pex8Δ and pex2Δ cells are comparable
TWO Pex13p degradation in H. polymorpha
56
(Figure 5), which may suggest that deleting PEX2 or PEX8 impacts on the same aspect
of Pex13p degradation, although further data will be required to validate this theory.
Deletion of PEX4 does not impact on Pex13p levels to the same extent as deletion of
a member of the peroxisomal E3 ligase complex (Figure 1). Pex13p degradation appears
completely blocked in pex2Δ cells (Figure 3), which leads us to conclude that Pex13p
degradation is not fully inhibited in cells lacking Pex4p. This could suggest that another
E2 enzyme, together with the peroxisomal E3 ligase complex, promotes Pex13p
ubiquitination and degradation in pex4Δ cells, albeit at an apparently lower level. While
we can only speculate as to the identity of the E2 in this model, the fact that Ubc4p has
been implicated in the ubiquitination and degradation of peroxisomal proteins and can
serve as E2 with the peroxisomal E3 ligase complex (El Magraoui et al, 2013; Platta et
al, 2009; Williams et al, 2008) makes it a possible candidate.
In summary, our results add strong support to the idea that the peroxisomal
ubiquitination machinery is not only required for ubiquitinating Pex5p and members of
the Pex20p family but also targets additional peroxisomal proteins. Indeed, members of
the peroxisomal E3 ligase complex are now linked to the ubiquitination/degradation of
Pex13p (this study), pexophagy induced Pex3p ubiquitination/degradation in H.
polymorpha (Williams & van der Klei, 2013b) and the ubiquitination of PMP70 in
mammals (Knoblach et al, 2013). In addition, Pex4p is required for the degradation of
the peroxisomal matrix proteins ICL and MLS in plants (Lingard et al, 2009), Pex18p
degradation in Saccharomyces cerevisiae (Purdue & Lazarow, 2001) and Pex20p
degradation in Pichia pastoris (Liu & Subramani, 2013) while when in complex with its
membrane anchor Pex22p, Pex4p from both S. cerevisiae and H. polymorpha is able to
produce K48 linked Ub chains in vitro (Kurochkin, 2005; Williams et al, 2012), which
suggests a role for Pex4p in proteasomal mediated degradation. However as with
Pex13p, further evidence that these proteins are bona fide substrates of the peroxisomal
ubiquitination machinery is still required. Nevertheless the results presented here,
together the above mentioned reports, lead us to propose that the peroxisomal
ubiquitination machinery, rather than simply being involved in receptor recycling, in fact
functions as a platform that facilitates the ubiquitination of an array of peroxisomal
proteins, regulating peroxisome biology through the ubiquitination/degradation of
peroxisomal proteins. Therefore, we anticipate that many more substrates of this
machinery remain to be discovered.
Pex13p degradation in H. polymorpha TWO
57
Materials and Methods
Molecular techniques and construction of H. polymorpha strains
Transformation of H. polymorpha was performed by electroporation as described
previously (Faber et al, 1994). H. polymorpha strains used in list study are listed in
Table 1. The plasmids and primers used in this study are listed in Table 2 and 3
respectively. Phusion DNA polymerase (Thermo Scientific) was used to produce gene
fragments.
The E. coli vector for expression of the SH3 domain of Pex13p, complete with
N-terminal His6- tag (pCW360) was made as follows: PCR was performed on H.
polymorpha genomic DNA using the primer combinations P13 SH3 F and P13 SH3 R,
the resulting fragment was digested with NcoI and HindIII and ligated into NcoI-HindIII
digested pETM11.
The H. polymorpha aox strain was made by Gateway cloning (Invitrogen). The
5’fragment of the AOX promoter (AOXp) was amplified with from genomic DNA using
primers attAOXp- 5’ UP and attAOXp- 5’ DN. The 3’fragment of AOXp, complete with
start of the coding region on the AOX gene was amplified with H. polymorpha genomic
DNA and primers att-AOX- 3’ UP and att-AOX- 3’ DN. Each PCR product was used for
the BP reaction to ligate into pENTR to generate pENTR-AOXp and pENTR-3’AOXp.
Plasmids pENTR-AOXp, pENTR-URA, pENTR-3’AOXp and pDEST-R4R3 were used
for LR reaction to generate pDEST-deltaAOX(URA). The product was digested with
PstI and BglII to generate two fragments of 2.3kb and 2.5kb. The 2.3kb fragment was
used for H.polymorpha transformation.
To construct pHIPZ20-mGFP, the PEX13 promoter (PPEX13) was amplified from
WT genomic DNA with primers Pro-P13-NotI-F and Pro-P13-SalI-R, and cloned into
pHIPZ6-Pex3-His6 (Williams & van der Klei, 2013b) replacing the PPEX3-Pex3-His6
fragment between NotI and SalI sites to generate pHIPZ20. mGFP was amplified from
Pex13-mGFP with primers SalI-GFP-F and GFP-XbaI-R and cloned into pHIPZ20
between SalI and XbaI sites. To construct pHIPZ20-Pex13-His6, a Pex13 fragment of
was amplified from WT genomic DNA with primers SalI-P13-F and P13-His6-XbaI-R,
which incorportated a sequence encoding for a C-terminal His6 tag into the DNA
fragment, and cloned into pHIPZ20-mGFP, replacing mGFP between the SalI and XbaI
sites. All plasmids containing PPEX13 were linearized with NheI prior to transformation
into H. polymorpha cells.
The plasmid pHIPH-Pex14-mKate2 was constructed as follows: PCR was
performed on the plasmid pFA6 yomKate2-CaURA3 (Addgene plasmid # 44878) using
primers yomKate2 fw and yomKate2 rev and the resulting mKate2 DNA fragment was
TWO Pex13p degradation in H. polymorpha
58
digested with BglII and SphI and ligated into BglII-SphI digested pSNA12 (Cepinska et
al, 2011), producing pHIPZ-Pex14-mKate2. This vector was linearized with PstI and
transformed into H. polymorpha WT cells. Next, genomic DNA was isolated from WT
Pex14-mKate2 (Zeo) cells and used as template for a PCR reaction using primers
Pex14-F and Pex14-SpeI-R and the DNA fragment was digested with BamHI and XmaI
and ligated into BamHI-XmaI digested pSEM04 (Knoops et al, 2014), producing
pHIPH5-Pex14-mKate2. This vector was then digested with NotI and BamHI to remove
AMO promoter fragment and the product was treated with Klenow fragment to produce
blunt-ends. Following this, the blunt ends were ligated together, forming the plasmid
pHIPH-Pex14-mKate2. pHIPH-Pex14-mKate2 was linearized with Bpu1102I prior to
transformation into H. polymorpha cells.
The pHIPZ-Pex13-mGFP plasmid (Knoops et al, 2014) was linearized with ApaI
prior to transformation into H. polymorpha cells.
All integrations were confirmed by colony PCR using Phire Hot Start II (Thermo
Scientific) and pex2 pHIPZ20-mGFP, pex4 pHIPZ20-mGFP, pex5 pHIPZ20-mGFP,
pex8 pHIPZ20-mGFP, pex14 pHIPZ20-mGFP, Myc-Ub-K48R pHIPZ20-mGFP, WT
pHIPZ20-mGFP and PEX13-His6 were further checked with Southern blotting.
Southern blotting
Southern blotting analysis was performed using the ECL Direct Nucleic Acid Labelling
and Detection system (Thermo Scientific) according to the established methods. H.
polymorpha genomic DNA containing the integrated plasmid PHIPZ20-mGFP was
digested with NdeI (Thermo Scientific) while H. polymorpha genomic DNA containing
the integrated pHIPZ20-Pex13-His6 plasmid was digested with EcoRI (Thermo
Scientific). The probe for PPEX13-mGFP, consisting of a 0.5 kb fragment upstream to
PEX13, was amplified using Pp13GFP-S-ProbeF and Pp13GFP-S-ProbeR. The probe
for Pex13-His6, consisting of a 0.5 kb fragment 1 kb-upstream, was amplified using
primers Sthn-13(R)CSProbF and Sthn-13(R)CSProbR. The probe recognises a 2.5 kb
fragment in pex13Δ cells and an ~8 kb fragment in one-copy mutant cells.
Strains and growth conditions
Yeast transformants were selected on YPD plates containing 2% agar and 100 μg/ml
Zeocin (Invitrogen) or 300 μg/ml Hygromycin (Invitrogen) or on YND plates containing
2% agar, for production of the aox deletion strain. The E. coli strain DH5α was used for
cloning purposes. E. coli cells were grown in LB supplemented with 100 μg/ml
Ampicillin at 37 °C. H. polymorpha cells were grown in batch cultures at 37 °C on
Pex13p degradation in H. polymorpha TWO
59
mineral media supplemented with 0.25% glucose or 0.5% methanol with 0.05% glycerol
as carbon source and 0.25% ammonium sulphate or 0.25% methylamine as nitrogen
source. Leucine, when required, was added to a final concentration of 30 μg/ml.
Cycloheximide (CHX) when used, was added to a final concentration of 6 mg/ml.
Preparation of yeasts TCA lysates
Cell extracts of TCA-treated cells were prepared for SDS-PAGE as detailed previously
(Baerends et al, 2000). Equal amounts of protein were loaded per lane and blots were
probed with rabbit polyclonal antisera raised against the Myc tag (Santa Cruz Biotech,
sc-789), Pex13p (Figure S1), Pex14p (Komori et al, 1997), Pex11p (Knoops et al, 2014)
or pyruvate carboxylase 1 (Pyc1) (Fahimi et al, 1993) or mouse monoclonal antisera
raised against penta-His tag (Qiagen, 34660) or mGFP (Santa Cruz Biotech, sc-9996).
Secondary goat anti-rabbit (31460) or goat anti-mouse (31430) antibodies conjugated to
horseradish peroxidase (Thermo Fisher Scientific) were used for detection. Pyc1 was
used as a loading control. Note that the anti-Pex14p can recognise both the
phosphorylated (upper band) and unphosphorylated (lower band) forms of Pex14p.
Expression and purification of Pex13p SH3 for antibody production
The SH3 domain of H. polymorpha Pex13p with a cleavable His6- tag was produced in
the E. coli strain BL21 (DE3) RIL. Cells were grown at 37°C to an OD600 of 1.0 in
Terrific Broth (TB) medium supplemented with antibiotics, transferred to 20°C and
grown until an OD600 of 1.5. Protein expression was then induced with 0.04mM IPTG
(Invitrogen) for 16 hrs and cells were harvested by centrifugation. E. coli cell pellets
expressing His6-Pex13 SH3 were thawed in lysis buffer (50 mM Tris-HCl pH 7.5, 300
mM NaCl, 10 mM Imidazole, 2 mM β-mercaptoethanol) and passed through a French
press. Cell debris was removed by centrifugation and lysates were loaded onto
glutathione Ni-NTA resin (Fisher Scientific) pre-equilibrated with lysis buffer. The resin
was extensively washed with lysis buffer, wash buffer 1 (50mM Tris,1M NaCl, 20 mM
Imidazole and 1 mM β-mercaptoethanol) and wash buffer 2 (50 mM Tris, 300 mM NaCl,
40 mM Imidazole and 1mM β-mercaptoethanol) and His6-Pex13 SH3 was eluted with
elution buffer (50 mM Tris, 150 mM NaCl, 330 mM imidazole and 1mM
β-mercaptoethanol). Finally, purified His6-Pex13 SH3 was passed over a PD10 column
(GE Healthcare) equilibrated in PD10 buffer (50 mM Tris, 150 mM NaCl and 1mM
β-mercaptoethanol) to remove the imidazole. After confirming presence of the purified
protein using SDS-PAGE, protein samples were sent for antibody production
(Eurogentec). The properties of the resulting anti-Pex13p antibodies are shown in Figure
TWO Pex13p degradation in H. polymorpha
60
S1.
Quantification of Western blots
Blots were scanned by using a densitometer (GS-710; Bio-Rad Laboratories) and
protein levels were quantified using Image Studio Lite Ver5.2 software (LI-COR
Biosciences). In the case of Pex14p blots, both the phosphorylated and
unphosphorylated forms were included in the calculation if both forms were visible. The
value obtained for each band was normalized by dividing it by the value of the
corresponding Pyc band (loading control). For comparison of absolute protein levels
(Figures 1 and 5), normalized values obtained for Pex13p, Pex14p and Pex11p levels in
WT cells were set to 1 and the levels of these proteins in mutant cells are displayed
relative to WT. For CHX experiments (Figures 2 and 3), the normalized values of T0
samples were set to 1.0 and values obtained from the T1-T3 samples are displayed as a
fraction of T0 values. Standard deviations were calculated using Excel. Significance was
determined using IBM SPSS Statistics 23 software (IBM), employing the function
analyse-compare means-independent samples t-test (with Levene test for deviation
homogeneity). * represents P-values < 0.05, ** represents P-values < 0.01 and ***
represents P-values < 0.001. The data presented are derived from three independent
experiments.
Pull-down assay
Cells were grown at 37°C to the mid-exponential growth phase (~8 hrs) in 200 mL
mineral medium containing 0.5% methanol and 0.05% glycerol and fifty OD600 units of
cells of each strain were harvested by centrifugation. Cells were washed once with
demineralized water and resuspended in Equilibrium buffer (50 mM potassium
phosphate buffer pH7.2, 10 mM imidazole, 10 mM iodoacetamide, 5 mM
N-ethymaleimide, 1 mM PMSF added just prior to use, and 2.5 μg/mL leupeptin). The
preparation of crude extracts of yeast cells using glass beads was performed as
previously described (Waterham et al, 1994). Samples of cell homogenates were then
treated for 30 min at room temperature with final concentration of 8 M urea and 1.0%
Triton X-100 (Sigma) to denature proteins and solubilize membranes. Samples were
briefly centrifuged at 4000×g to remove unbroken cells and lysates were incubated with
Ni-NTA resin (QIAGEN) for 60 min at room temperature, with gentle shaking. The
resin was then sequentially washed with Wash buffer 1 (50 mM potassium phosphate
buffer pH7.2, 40 mM imidazole, 6 M urea, 10 mM iodoacetamide, 5 mM
N-ethymaleimide, 1 mM PMSF added just prior to use, and 2.5 μg/mL leupeptin) and
Pex13p degradation in H. polymorpha TWO
61
Wash buffer 2 (50 mM potassium phosphate buffer pH7.2, 40 mM imidazole, 6 M urea,
1.0% Triton X-100, 10 mM iodoacetamide, 5 mM N-ethymaleimide, 1 mM PMSF
added just prior to use, and 2.5 μg/mL leupeptin). The resin was then transferred to new
tube, all liquid was removed with syringe and proteins were eluted with SDS-PAGE
loading buffer (without β-mercaptoethanol) at 37°C for 10 min.
Fluorescence Microscopy
All fluorescence microscopy images were acquired using a 100×1.30 NA Plan-Neofluar
objective (Carl Zeiss). Wide-field microscopy images were captured by an inverted
microscope (Axio Scope A1, Carl Zeiss) using Micro-Manager software and a digital
camera (CoolSNAP HQ2; Photometrics). GFP signal was visualized with a 470/440-nm
band pass excitation filter, a 495-nm dichromatic mirror, and 525/550-nm band pass
emission filter.
For images taken of Pex13-mGFP in WT grown on methanol/glycerol mineral
medium, the optimal settings were mGFP (255, 2500) and mKate2 (219, 3000), and in
pex2, the optimal settings mGFP (255, 7000) and mKate2 (219, 4700) were applied for
processing. The general settings used to compare the signal of Pex13-mGFP in WT and
pex2, mGFP (255, 5000) and mKate2 (219, 4000) were applied for processing.
For quantification of the Pex13-mGFP signal in WT or pex2 cells, a rectangular
area was drawn using the “rectangular tool” from ImageJ (Abramoff et al, 2004) to
envelope the region containing the Pex13-mGFP spot and pixel intensity inside the area
was measured. The measured maximum fluorescence intensity of GFP on peroxisomes
was corrected for the background intensity and a box plot was made using Microsoft
Excel. The box represents values from the 25 percentile to the 75 percentile; the
horizontal line through the box represents the median value. Whiskers indicate
maximum and minimum values. The intensity ratio of mGFP/ mKate was calculated
based on the same cells from Figure 6C. The maximum intensity of Pex13-mGFP was
divided by the corresponding maximum intensity of Pex14-mKate2 in each cell. The
dataset was subjected to the two-tail t-test using Microsoft Excel 2010. * represents
P-values < 0.05, ** represents P-values < 0.01 and *** represents P-values < 0.001.
Acknowledgements
The authors thank Ida van der Klei, Thomas Schroeter, Jessica Kluemper, Wolfgang
Schliebs and Ralf Erdmann for helpful discussions, Arjen Krikken for advice with
processing of fluorescence microscopy images and Jan Kiel for critically reading the
manuscript. This work was funded by a VIDI Fellowship (723.013.004) from the
TWO Pex13p degradation in H. polymorpha
62
Netherlands Organisation for Scientific Research (NWO), awarded to CW.
Conflict of interest
The authors declare no conflict of interest.
Figure S1. Specificity of H. polymorpha Pex13p antibodies.
Western blots of lysates of WT and pex13 cells probed with pre-immune sera (left panel) or
sera isolated from a rabbit immunogenized with the purified SH3 domain of Pex13p (right
panel). * Denotes anti-Pex13p cross reactive species.
Pex13p degradation in H. polymorpha TWO
63
Table 1, H. polymorpha strains used in this study
Strain Description Reference
WT Hp WT (NCYC495), leu1.1 (Gleeson
&
Sudbery,
1988)
Myc-Ub-K48R Hp WT with pRDV2 (hygR), leu1.1 (Williams
& van der
Klei,
2013b)
WT Pex14-mKate2 (Zeo) Hp WT with pHIPZ-Pex14-mKate2
(zeoR)
This study
WT Pex13-mGFP Hp WT with pHIPZ-Pex13-mGFP
(zeoR), leu1.1
This study
Myc-Ub-K48R Pex13-mGFP Hp WT with pRDV2 (hygR) and
pHIPZ-Pex13-mGFP (zeoR), leu1.1
This study
pex2 pex2 disruption strain, leu1.1 (Koek et
al, 2007)
pex10 pex10 disruption strain (Tan et al,
1995)
pex12 pex12 disruption strain, leu1.1 (Koek et
al, 2007)
pex4 pex4 disruption strain, leu1.1 (Van der
Klei et al,
1998)
pex13 pex13 disruption strain, leu1.1 (Koek et
al, 2007)
pex5 pex5 disruption strain, leu1.1 (Van der
Klei et al,
1995)
pex14 pex14 disruption strain, leu1.1 (Komori
et al,
1997)
pex20 pex20 disruption strain, leu1.1 (Otzen et
al, 2005)
TWO Pex13p degradation in H. polymorpha
64
pex7 pex7 disruption strain, leu1.1 (Koek et
al, 2007)
pex8 pex8 disruption strain, leu1.1 (Haan et
al, 2002)
aox Hp NCYC deltaAOX (AOX::URA),
leu1.1
This study
atg1 Hp atg1 deletion strain, leu1.1 (Nakai,
2007)
pex2 Pex13-mGFP+
Pex14-mKate2 (Hyg)
pex2 with pHIPZ-Pex13-mGFP (zeoR)
and pHIPH-Pex14-mKate2 (hygR), leu1.1
This study
pex2 + Pex13-mGFP pex2 with pHIPZ-Pex13-mGFP (zeoR),
leu1.1
This study
WT Pex13-mGFP+
Pex14-mKate2 (Hyg)
WT with pHIPZ-Pex13-mGFP (zeoR)
and pHIPH-Pex14-mKate2 (hygR), leu1.1
This study
WT + Pex13-mGFP WT with pHIPZ-Pex13-mGFP (zeoR),
leu1.1
This study
pex2 PPEX13 mGFP Δpex2 with pHIPZ20 mGFP (zeoR),
leu1.1
This study
pex4 PPEX13 mGFP Δpex4 with pHIPZ20 mGFP (zeoR),
leu1.1
This study
pex5 PPEX13 mGFP Δpex5 with pHIPZ20 mGFP (zeoR),
leu1.1
This study
pex8 PPEX13 mGFP Δpex8 with pHIPZ20 mGFP (zeoR),
leu1.1
This study
pex14 PPEX13 mGFP Δpex14 with pHIPZ20-mGFP (zeoR),
leu1.1
This study
Myc-Ub-K48R PPEX13 mGFP Myc-Ub-K48R with pHIPZ20-mGFP
(zeoR , leu1.1
This study
WT PPEX13 mGFP WT with pHIPZ20-mGFP (zeoR), leu1.1 This study
Pex13-His WT with pHIPZ20-Pex13-His6 (zeoR),
leu1.1
This study
Pex13-His/Myc-Ub pex13 with pHIPZ20-Pex13-His6 (zeoR)
and pRDV1 (hygR), leu1.1
This study
pex2/Myc-Ub pex2 with pRDV1 (hygR), leu1.1 This study
pex2/Pex13-His pex2 with pHIPZ20-Pex13-His6 (zeoR),
leu1.1
This study
Pex13p degradation in H. polymorpha TWO
65
pex2/Pex13-His/Myc-Ub pex2 with pHIPZ20-Pex13-His6 (zeoR)
and pRDV1 (hygR), leu1.1
This study
Table 2, plasmids used in this study
Plasmid Description Reference
pETM11 N-terminal His6 tag, kanR EMBL
collection#
pCW360 Pex13-SH3 domain with N-terminal His6 tag
for E. coli expression, kanR
This study
pRDV1 Myc tagged ubiquitin under control of
DHAS promoter, zeoR
; ampR
(Williams &
van der Klei,
2013b)
pRDV2 Myc tagged ubiquitin mutate (Ub-K48R)
under control of DHAS promoter, zeoR
;
ampR
(Williams &
van der Klei,
2013b)
pHIPZ6-Pex3-His6 Pex3-His6 under control of its endogenous
promoter, zeoR
(Williams &
van der Klei,
2013b)
pHIPZ-Pex13-mGFP C-terminal part of Pex13 fused with mGFP,
zeoR
; ampR
(Knoops et
al, 2014)
pSNA12 C-terminal part of Pex14 fused with mGFP,
zeoR
; ampR
(Cepinska et
al, 2011)
pHIPZ-Pex14-mKate2 Plasmid containing the C-terminal region of
H. polymorpha PEX14 fused to mKate2;
hygR
; ampR
This study
pSEM04 Plasmid containing PEX3 under control of
the AMO promoter, hygR, amp
R
(Knoops et
al, 2014)
pHIPH5-Pex14-mKate2 Plasmid containing the full length H.
polymorpha PEX14 fused to mKate2, under
control of the AMO promotor, hygR
; ampR
This study
pHIPH-Pex14-mKate2 Plasmid containing the C-terminal region of
H. polymorpha PEX14 fused to mKate2;
hygR
; ampR
This study
pDEST-deltaAOX(URA) pDEST vector containing URA fragment This study
TWO Pex13p degradation in H. polymorpha
66
with regions homologous to 5’ and 3’
regions of AOX gene, ampR
pHIPZ20 Plasmid containing PEX13 endogenous
promoter, zeoR
; ampR
This study
pHIPZ20-mGFP mGFP under control of PEX13 promoter,
zeoR
; ampR
This study
pHIPZ20-Pex13-His6 Pex13 fused to a 6*His tag at its C-terminus,
under control of PEX13 promoter, zeoR
;
ampR
This study
#https://www.embl.de/pepcore/pepcore_services/cloning/choice_vector/ecoli/embl/popu
p_emblvectors/
Table 3, primers used in this study
Primer Sequence Description
P13 SH3 F GCGCCCATGGAGTTTGCGC
GGGCGCTATC
To clone the Pex13 SH3 domain,
forward primer
P13 SH3 R CGCGAAGCTTTAGATCAAT
AGCTTTTGATCTTTCTTG
To clone the Pex13 SH3 domain,
reverse primer
SalI-P13-F ACGCGTCGACATGACTACA
CCACGTCCAAAG
To clone the Pex13 gene,
forward primer
P13-His6-XbaI-R CTAGTCTAGATCAGTGATG
GTGATGGTGATGGATCAAA
AGCTTTTGATCTTTCTTG
To clone the Pex13 gene with
His6 tag, reverse primer, used to
make construct
pHIPZ20-Pex13-His6
Sthn-13(R)CSPro
bF
CAACAACGAATCTAGATTC
AAGAC
To clone the probe for Pex13-His
Southern blotting, forward
primer
Sthn-13(R)CSPro
bR
TCGTTACCTGTGATGCTACA
G
To clone the probe for Pex13-His
Southern blotting, reverse primer
attAOXp-5’ UP GGGGACAACTTTGTATAGA
AAAGTTGTCTGCAGCCGCA
ACCGAACTTTTCGC
To clone the 5’ fragment of AOX
promoter, forward primer, used
to make aox
attAOXp- 5’ DN GGGGACTGCTTTTTTGTACA
AACTTGGATTGATGTCACC
To clone the 5’ fragment of AOX
promoter, reverse primer, used to
Pex13p degradation in H. polymorpha TWO
67
ACCGTGCACTGGC make aox
attAOXp- 3’ UP GGGGACAGCTTTCTTGTAC
AAAGTGGTTCCACGTGACC
TCCAACCAAGTCC
To clone the 3’ fragment of AOX
promoter and N-terminal,
forward primer, used to make
aox
attAOXp- 3’ DN GGGGACAACTTTGTATAAT
AAAGTTGTTAGAATCTGGC
AAGTCCGGTCTCC
To clone the 3’ fragment of AOX
promoter and N-terminal, reverse
primer, used to make aox
Pro-P13-NotI-F ATAAGAATGCGGCCGCGCT
TAAATTTTCAAAGCTCCAA
G
To clone the Pex13 endogenous
promoter, forward primer
Pro-P13-SalI-R ACGCGTCGACGGAAGAACG
ATTTTCTTGTTTTTTTTC
To clone the Pex13 endogenous
promoter, reverse primer, used to
make construct pHIPZ20-mGFP
SalI-GFP-F ACGCGTCGACATGGTGAGC
AAGGGCG
To clone the mGFP fragment
with start codon, forward primer
GFP-XbaI-R CTAGTCTAGATCACTTGTAC
AGCTCGTCCATG
To clone the mGFP fragment
with stop codon, reverse primer
yomKate2 fw CGCAGATCTATGGTTTCTGA
ACTCATCAAG
To clone mKate2 fragment,
forward primer
yomKate2 rev CTAAGTTGGGACACAGATA
AGCATGCCGC
To clone mKate2 fragment,
reverse primer
Pp13GFP-S-Probe
F
TCAAGCAGTTCTTCTGTAGC
ATC
To clone the probe for
PPEX13-mGFP Southern blotting,
forward primer
Pp13GFP-S-Probe
R
GTCTTGAGCAGCGGTCTC To clone the probe for
PPEX13-mGFP Southern blotting,
reverse primer
Pex14-F GTCCTTCATATCGTACAGG
ATCCATGTCTCAACAGCCA
GCAACGACC
To clone the Pex14-mKate2,
forward primer, used to make
construct
pHIPH5-Pex14-mKate2
Pex14-SpeI-R GAAGGCTGGATGTCCAGGC
CCGGGTTACCGGTGTCCCA
ACTTAGATGGCAAATCACA
G
To clone the Pex14-mKate2,
reverse primer, used to make
construct
pHIPH5-Pex14-mKate2
68
3
Chapter 3
Further insights into Pex13p degradation in the yeast Hansenula polymorpha
Xin Chen and Chris Williams
Author contributions
CW supervised the project. CW and XC conceived the project and designed the
experiments. XC and CW analysed the data. XC performed biochemical and FM
experiments. XC and CW wrote the manuscript.
THREE Further insights into Pex13p degradation
70
Further insights into Pex13p degradation in the yeast Hansenula polymorpha
Xin Chen1 and Chris Williams
1,*
1Cell Biochemistry, Groningen Biomolecular Sciences and Biotechnology Institute,
University of Groningen, 9747AG, the Netherlands
Abstract
The peroxisomal membrane protein Pex13p is required for the import of matrix proteins
into peroxisomes. Previously we reported that Pex13p in the yeast Hansenula
polymorpha undergoes rapid degradation. Furthermore, H. polymorpha Pex13p is
ubiquitinated and degraded in a process that requires the peroxisomal E3 ligase Pex2p.
However, the underlying reason why Pex13p undergoes degradation remained unknown.
Therefore, we sought to shed light on the function of Pex13p degradation in H.
polymorpha. In this study, we demonstrate that Pex2p-dependent turnover of Pex13p
also occurs under peroxisome non-inducing condition, demonstrating that Pex13p
degradation is a general and not a media-specific event. Furthermore, we show that
blocking the recycling of the type 1 peroxisomal matrix protein receptor Pex5p led to
increased Pex13p levels, suggesting Pex5p recycling is linked to Pex13p degradation.
Additionally, we identify a Pex13p mutant that is inhibited in degradation. We
demonstrate that inhibiting Pex13p degradation can impact negatively on the ability of
cells to grow on methanol-containing media. Based on our results, we discuss possible
functions of Pex13p degradation in relation to peroxisomal matrix protein import.
Keywords: Peroxisome/ protein degradation/ Hansenula polymorpha/ PMP/ Pex13p
Further insights into Pex13p degradation THREE
71
Introduction
The peroxisome is a single membrane bounded compartment present in the cytoplasm of
nearly all eukaryotes that plays an essential role in cellular metabolism (Gabaldon,
2010). Many metabolic processes can be found in peroxisomes, depending on organism
and cell type. A few examples include the decomposition of fatty acids in mammalian
cells and the yeast Saccharomyces cerevisiae (Lazarow, 1978; Van Roermund et al,
1998), the biosynthesis of plasmalogens in mammalian cells (Zoeller et al, 1992), the
reduction of reactive oxygen species, especially hydrogen peroxide (Bonekamp et al,
2009; Wanders & Waterham, 2006), the synthesis of penicillin in the fungus Penicillium
chrysogenum (Kiel et al, 2005c) and the oxidation of methanol in the yeast Hansenula
polymorpha (Van Dijken et al, 1975). However, there are many more. Dysfunctional
peroxisomes are known to cause a spectrum of physiological, often fatal disorders in
humans (Waterham et al, 2016), demonstrating their importance in cellular metabolism.
The soluble proteins inside the peroxisomal matrix, most often enzymes, determine
the function of the peroxisome. All peroxisomal matrix proteins are made in the cytosol
and imported post-translationally, through the aid of a peroxisomal targeting signal (PTS)
(Hasan, 2013). A minor portion of matrix proteins contain an N-terminal PTS2 signal
(Lazarow, 2006) whereas most peroxisomal matrix proteins harbour a PTS1 signal at the
C-terminus of the protein (Miura et al, 1992). Each PTS requires a separate receptor that
binds to the PTS and transports the PTS-containing cargo protein to the peroxisome. For
PTS1 containing proteins Pex5p acts as receptor whereas PTS2-containing proteins
require a protein complex, consisting of the cargo-binding protein Pex7p and a
co-receptor protein, which in yeast is a member of the Pex20p family and in mammalian
cells is an isoform of Pex5p (Dodt & Gould, 1996; Sichting et al, 2003). After binding
the cargo in the cytosol, the receptors transport the cargo to the peroxisomal membrane,
where they come into contact with the docking complex, consisting of Pex14p, Pex13p
and, in yeast, Pex17p (Hasan, 2013; Johnson et al, 2001; Snyder et al, 1999). Next, the
cargo is translocated into the peroxisomal matrix in a process that is not well understood
but one that likely requires the action of the intra-peroxisomal protein Pex8p (Agne et al,
2003; Rehling et al, 2000a). Finally, the receptors are ubiquitinated and recycled to the
cytosol by the AAA-ATPases Pex1p and Pex6p (Platta et al, 2008).
Ubiquitination is a post-translational modification involving the attachment of
ubiquitin, a 76-amino acid globular protein, to a substrate protein (Hershko, 1996).
Ubiquitination occurs in three steps; first ubiquitin is activated by the ubiquitin
activating enzyme (E1) with the consumption of ATP. Next, ubiquitin is transferred to a
ubiquitin-conjugating enzyme (E2) and finally, with the help of either a HECT ubiquitin
THREE Further insights into Pex13p degradation
72
ligase (HECT E3), which conjugates ubiquitin in much the same way as an E2, or a
RING E3, which functions as a bridge between E2 and the substrate, the ubiquitin is
conjugated to the substrate (Scheffner et al, 1995). The number of E1, E2 and E3
enzymes varies from organism to organism but a pyramidal structure is common, with a
single E1, tens of E2s and up to a hundred or more E3s (Hershko & Ciechanover, 1998).
Protein ubiquitination serves many functions and the particular function often depends
on the number of ubiquitin molecules attached to a substrate (Sadowski et al, 2012). The
attachment of a chain of ubiquitin molecules to a substrate, referred to as
poly-ubiquitination, often targets substrates for degradation by the proteasome whereas
the attachment of one or two ubiquitin molecules, often called mono-ubiquitination, is
usually for non-proteolytic functions (Polo et al, 2002; Yau & Rape, 2016).
The receptor protein Pex5p can be ubiquitinated in two ways, resulting in different
outcomes. Pex5p can be mono-ubiquitinated on a conserved cysteine close to the
N-terminus or poly-ubiquitinated on lysine residues downstream of the cysteine (Kiel et
al, 2005b; Platta et al, 2004; Williams et al, 2007). Pex5p mono-ubiquitination requires
the E2 Pex4p and the peroxisomal E3 ligase complex, consisting of the RING E3s
Pex2p, Pex10p, Pex12p and plays a role in Pex5p recycling (Grou et al, 2009; Platta et
al, 2007; Williams et al, 2007). On the other hand, Pex5p poly-ubiquitination is
performed by the E2 Ubc4p, together with the peroxisomal E3 ligase complex, resulting
in the degradation of Pex5p via the proteasome (Kiel et al, 2005a; Platta et al, 2004).
In all organisms to date, the PMP Pex13p was shown to play an essential role in the
import of matrix proteins containing either a PTS1 or a PTS2 because cells depleted of
Pex13p exhibit a matrix protein import defect (Cross et al, 2016; Toyama et al, 1999;
Williams & Distel, 2006). Pex13p is a member of the docking complex at the
peroxisomal membrane. The docking complex is composed of Pex14p and Pex13p (and
Pex17p in yeast, see below) and its function is to allow the cytosolic receptor proteins
carrying cargo to associate with the peroxisomal membrane (Hasan, 2013; Johnson et al,
2001; Snyder et al, 1999), although it is believed to also play a role in the cargo
translocation step (Girzalsky et al, 2010). Pex13p was the first PMP identified as
“docking factor” for the cycling receptors (Elgersma et al, 1996; Erdmann & Blobel,
1996; Gould et al, 1996). However, later data raised questions as to whether this simple
description was sufficient. The Pex5p-Pex14p interaction appears stronger in the
presence of a PTS1 cargo bound to Pex5p, whereas the Pex5p-Pex13p interaction
appears stronger in the absence of cargo (Otera et al, 2002; Urquhart et al, 2000).
Furthermore, the peroxisomal docking complex in yeast, in addition to Pex13p and
Pex14p, contains a third identified component, Pex17p (Snyder et al, 1999). Pex17p
Further insights into Pex13p degradation THREE
73
directly binds to Pex14p and, based on immunoprecipitation experiments, Pex14p and
Pex17p coprecipitate with both PTS receptors in the absence of Pex13p (Huhse et al,
1998). All these data have led to the conclusion that Pex14p is the first “point of
contact” at the peroxisomal membrane for the cargo-bound receptors and that Pex13p is
involved in the cargo translocation or receptor recycling steps of matrix protein import.
Nevertheless, further information on this is lacking (Williams & Distel, 2006). Recently,
it was reported that Pex13p is required for selective autophagy of Sindbis virus particles
(virophagy) and of damaged mitochondria (mitophagy) in mammalian cells but whether
this is linked to its role in peroxisomal matrix protein import or if it is a general function
of Pex13p is not known (Lassen & Xavier, 2018; Lee et al, 2017; Rahim et al, 2016).
Previously we demonstrated that H. polymorpha Pex13p is degraded via the
ubiquitin-proteasome system (UPS) in a Pex2p dependent manner (Chen et al, 2018).
However, the underlying reason why Pex13p undergoes rapid degradation remained
unknown. Therefore, we sought to shed further light on Pex13p degradation in H.
polymorpha. We demonstrate that Pex13p degradation is a general, rather than media
specific process and we provide evidence that links Pex5p recycling to Pex13p
degradation. In addition, we identify a Pex13p mutant that displays a reduced turnover
and elevated protein levels and, using this mutant, we demonstrate that inhibition of
Pex13p degradation can impact negatively on the ability of cells to grow on
methanol-containing media. Finally, we provide evidence that Pex14p levels play a
determining role in the degradation of Pex13p. We discuss our results in the context of
Pex13p and peroxisome function.
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Results
Pex13p has a relatively short half-life on glucose
Previously, we demonstrated that Pex13p undergoes rapid UPS-mediated degradation in
H. polymorpha cells grown on methanol, conditions which require peroxisome function
for growth (Chen et al, 2018). To determine whether Pex13p degradation is a methanol
specific or more general occurrence, we investigated Pex13p degradation in cells grown
on glucose, a condition where peroxisome function is not required for growth. We used
strains expressing Pex13p tagged with mGFP (Pex13-mGFP), to allow us to assess both
the degradation (with western blotting) and subcellular localization (with fluorescence
microscopy) of Pex13p. As with wild type (WT) Pex13p, Pex13-mGFP also undergoes
UPS-mediated degradation (Chen et al, 2018). To determine whether Pex13-mGFP is
actively degraded in cells grown on glucose, we assessed the stability of Pex13-mGFP in
both WT and pex2 (deletion of a ubiquitin ligase E3 PEX2) cells treated with
Cycloheximide (CHX). CHX is a ribosome inhibitor that blocks protein production and
then protein degradation in CHX-treated cells can be followed using western blotting.
We observed that Pex13-mGFP is actively degraded in WT cells grown on glucose, but
not in pex2 cells, establishing that Pex13-mGFP degradation occurs on glucose and
requires a functional peroxisomal E3 ligase complex (Fig. 1A-D). Furthermore,
Pex13-mGFP levels are elevated in pex2 and pex4 (Pex4p is a peroxisome-associated E2)
cells grown on glucose, relative to WT cells (Fig. 2A & B), similar to the results we
obtained with methanol-grown cells (Chen et al, 2018). Finally, we investigated where
Pex13-mGFP builds up in glucose-grown cells, when its degradation is inhibited.
According to our fluorescence microscopy images, Pex13-mGFP co-localizes with
Pex14-mKate2 (used here as marker for peroxisomes) in both WT and pex2 cells and
accumulates at the peroxisomal membrane in pex2 cells (Fig. 2C & D). Additionally,
pex2 cells displayed an increase in GFP intensity (Fig. 2E) as well as an increased
mGFP/mKate2 intensity ratio (Fig. 2F) compared to WT cells. These data demonstrate
that Pex2p-dependent Pex13p degradation occurs on glucose, establishing that it is a
general, rather than a methanol-specific process.
Pex13p degradation is linked to the recycling of Pex5p
Our previous data indicated that Pex13p degradation was inhibited in cells lacking
Pex5p, the PTS1 protein import receptor, but not in cells lacking Pex7p or Pex20p, the
PTS2 (co-)import receptors (Chen et al, 2018). This, coupled with the observation that
Pex13p degradation is a general process (see above), led us to suspect that Pex13p
degradation could be involved in the import of PTS1 proteins. Originally Pex13p was
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described as a docking factor for the cycling receptors (Elgersma et al, 1996; Erdmann
& Blobel, 1996; Gould et al, 1996). However, later reports demonstrated that Pex13p
binds more strongly to Pex5p when not in complex with a PTS1 cargo protein, whereas
the Pex5p-Pex14p interaction is enhanced when Pex5p is bound to a PTS1 protein
(Otera et al, 2002; Urquhart et al, 2000). In addition, Pex13p binds to Pex8p (Deckers et
al, 2010) and this interaction allows the docking complex, consisting of Pex13p, Pex14p
and Pex17p, to contact the peroxisomal E3 ligase complex, which is required for
receptor ubiquitination and the following recycling (Agne et al, 2003). Together, these
data suggest that Pex13p could play a role in Pex5p recycling. Therefore, we
investigated the link between Pex5p recycling and Pex13p degradation.
The recycling of Pex5p from the peroxisomal membrane requires Pex5p to be
mono-ubiquitinated by the E2 Pex4p on a conserved cysteine residue close to its
N-terminus (Grou et al, 2008; Platta et al, 2007; Williams et al, 2007). In cases where
Pex5p mono-ubiquitination in inhibited (through mutation of the conserved cysteine or
deletion of PEX4), Pex5p is poly-ubiquitinated on lysine residues in its N-terminal
region by the E2 Ubc4p and subsequently degraded via the proteasome (Kiel et al,
2005b; Williams et al, 2007). Inhibition of both Pex4p- and Ubc4p-dependent
ubiquitination causes a block in both Pex5p recycling and Pex5p degradation and
consequently a build-up of Pex5p on the peroxisomal membrane (Platta et al, 2008;
Platta et al, 2007). In H. polymorpha, the conserved residues are Cys-9 and Lys-21 (Kiel
et al, 2005b). To investigate the link between Pex5p recycling and Pex13p degradation,
we assessed the levels of Pex13p in cells expressing Pex5p point mutants blocking
either Pex5p recycling (Pex5-C9S), Pex5p degradation (Pex5-K21R) or both
(Pex5-C9S.K21R). In Pex5-K21R, the degradation is inhibited while the recycling is
still functional, and Pex5p level in this mutant is comparable to WT. As can be seen
from Fig 3, inhibition of Pex5p recycling results in increased Pex13p levels, an effect
that was enhanced when Pex5-C9S degradation was additionally blocked by the K21R
mutation (Fig. 3A,B). It is worthy to note here that Pex13p levels appear elevated in
pex5 cells, where no Pex5p is present and in Pex5-C9S.K21R cells, where Pex5p levels
are enhanced (see Fig. 3). Because of this apparent contradiction, we assessed Pex13p
levels in pex4 cells expressing Pex5-K21R. Both the Pex4p- and the Ubc4p-dependent
ubiquitination of Pex5p is inhibited in these cells, similar to in Pex5-C9S.K21R cells.
We observed that Pex13p levels were also elevated in pex4 cells expressing Pex5-K21R
(Fig. 3), validating the results obtained with Pex5-C9S.K21R cells. Together, our data
suggest that Pex13p degradation is functionally linked to Pex5p recycling.
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The PEST sequence in Pex13p is not required for its degradation
Pex13p is constitutively degraded in cells grown on glucose and on methanol containing
media while Pex14p, a Pex13p binding partner and fellow member of the docking
complex, is relatively stable under these conditions (see Fig. 1 and (Chen et al, 2018)).
This demonstrates that the levels of these two proteins are regulated differently and
could indicate that Pex13p contains a “degron” encoded in its sequence (Bachmair &
Varshavsky, 1989; Varshavsky, 1997). Such sequences facilitate protein degradation and
one well-studied degron is the PEST sequence. A PEST sequence is an unstructured
region in a protein rich in proline (P), glutamate (E), serine (S) and threonine (T)
residues that targets the protein for degradation (Rogers et al, 1986).
Analysing the H. polymorpha Pex13p sequence, we found a putative PEST
sequence in proximity to the N-terminus, based on the prediction program epestfind
(http://emboss.bioinformatics.nl/cgi-bin/emboss/epestfind), with a score of 13.1 (Fig.
4A). A score above 5 is considered significant. To investigate whether the putative PEST
sequence in Pex13p is involved in its degradation, we constructed a strain expressing
Pex13p deleted for the PEST sequence (Δpest), under control of its endogenous
promoter. Because we do not know which epitopes in Pex13p are recognized by our
Pex13p antibody, we also added a C-terminal His6 tag and followed the degradation of
WT and Δpest Pex13p using anti-His antibodies. We followed WT and Δpest
Pex13-His6 levels over-time in CHX treated cells grown on methanol media containing
(Fig. 4B-E). However, the removal of the putative PEST sequence in Pex13p did not
inhibit Pex13p turnover, suggesting that it is not involved in Pex13p degradation.
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Fig. 1 Pex13-mGFP degradation occurs in H. polymorpha cells grown on glucose.
A WT cells expressing Pex13-mGFP were grown on glucose media for 4 hrs and treated
with DMSO (Ctrl) or Cycloheximide (CHX). TCA samples were taken at the indicated
time (hrs) after DMSO/CHX addition and probed by SDS-PAGE and immunoblotting
with antibodies against mGFP, Pex14p and Pyc.
B Representative western blots of pex2 cells expressing Pex13-mGFP derived from cells
grown and treated as in A. Samples were probed with SDS-PAGE and immunoblotting
with antibodies against mGFP, Pex14p and Pyc.
C Quantification of Pex13-mGFP levels in WT and pex2 cells expressing Pex13-mGFP.
Protein levels were normalized to the loading control Pyc at the corresponding time
point. Protein levels at T0 were set to 1. Values represent the mean ± SD of three
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independent experiments. The asterisks denotes statistically significant differences in
protein levels compared to those in WT samples (*P < 0.05, **P < 0.01).
D Quantification of Pex14p levels in WT and pex2 cells expressing Pex13-mGFP. Protein
levels were normalized to Pyc at the corresponding time point. Protein levels at T0 were
set to 1. Values represent the mean ± SD of three independent experiments.
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Fig. 2 Pex13-mGFP accumulates on peroxisomes in H. polymorpha pex2 cells grown
on glucose.
A WT and pex2 cells producing Pex13-mGFP were grown on glucose media and TCA
samples were taken when the cultures reached an OD600 of 1.0. Samples were subjected
to SDS-PAGE and immunoblotting using antibodies against mGFP, Pex14p and Pyc.
B Quantification of protein levels in WT and mutant cells, normalized to the loading
control Pyc. Protein levels in WT cells were set to 1. Values represent the mean ± SD of
three independent experiments. An Asterisks denotes statistically significant increases in
protein levels compared to those in WT samples (*P < 0.05, **P < 0.01).
C WT and pex2 cells producing Pex13-mGFP and Pex14-mKate2 were grown on glucose
media to an OD600 of 1.0 and fluorescence microscopy images were taken. Images of
Pex13-mGFP were processed using ImageJ with optimal settings to show signals in WT
and pex2 cells. Pex14-mKate2 was used as peroxisomal membrane marker. The
following settings were used: for WT cells mGFP (255, 800) and mKate2 (219, 1200);
for pex2 cells mGFP (255, 3000) and mKate2 (219, 2200). Scale bar: 5μm.
D Fluorescence images of Pex13-mGFP in WT or pex2 cells shown in (A) were processed
using ImageJ with the same settings: mGFP (255, 2000), mKate2 (219, 1700). Scale bar:
5μm.
E Box plot showing quantification of mGFP and mKate2 fluorescence intensity at the
peroxisomal membrane in WT and pex2 cells producing Pex13-mGFP and
Pex14-mKate2. Fluorescence intensities (auxiliary units) were measured using ImageJ.
The box represents values from the 25 percentile to the 75 percentile; the horizontal line
through the box represents the median value. Whiskers indicate maximum and minimum
values. mGFP and mKate2 measurements were taken as described in the Materials and
Methods section.
F Average ratio ± SD of mGFP to mKate intensities in 40 WT and pex2 cells. *P<0.1, **P
< 0.01.
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Fig. 3 Pex13p degradation is linked to the recycling of Pex5p.
A Representative western blots of samples derived from WT and mutant cells grown for 14
hrs on methanol/glycerol media. Blots were probed with antibodies directed against
Pex5p, Pex13p, Pex14p, Pex11p and Pyc. * Denotes anti-Pex13p cross reactive species.
B Quantification of protein levels in WT and mutant cells, normalized to the loading
control Pyc at the corresponding time point. Protein levels in WT cells were set to 1.
Values represent the mean ± SD of three independent experiments. Asterisks denote
statistically significant increases in protein levels compared to those in WT samples (*P
< 0.05, **P < 0.01, ***P < 0.001).
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The N-terminus and lysine residues are involved in Pex13p degradation
Because deletion of the putative PEST sequence in Pex13p did not impact on Pex13p
turnover (see Fig. 4), we sought an alternative method to inhibit Pex13p degradation, to
investigate the role of Pex13p degradation in matrix protein import. Previously we
reported that Pex13p is ubiquitinated (Chen et al, 2018) and because protein
ubiquitination usually occurs on NH2 groups in the protein (Chau et al, 1989;
Ciechanover & Ben-Saadon, 2004), our strategy was to block NH2 groups in Pex13p. To
achieve this, we developed several Pex13p constructs in which the NH2 groups were
blocked. One construct had all lysines replaced by arginine residues (Pex13-KR).
Another construct contained the amino acids serine and glutamic acid directly after the
start codon (Pex13-NT), which was predicted to result in the acetylation of the
N-terminal NH2 group and therefore block ubiquitin attachment (Kiemer et al, 2004;
Perrot et al, 2008). The final construct was the combination of the previous two, with
both lysine residues and the N-terminal NH2 group blocked (Pex13-KRNT). Similar to
our Pex13 Δpest construct, all NH2 blocking constructs contained a His6 tag, either at
the N-terminal (Pex13-NT, Pex13-KRNT) or C-terminal (Pex13, Pex13-KR) and protein
levels were probed using anti-His6 antibodies, to rule out any potential differences in the
way in which the Pex13p antibodies may recognize the different versions of Pex13p.
Our data demonstrate that Pex13-His6 levels were comparable in cells expressing
Pex13-KR, Pex13-NT and WT forms of Pex13-His6 grown on methanol containing
media (Fig. 5A & B), suggesting that blocking the N-terminus or lysine residues was
insufficient to inhibit Pex13p degradation. However, Pex13-His6 levels were
dramatically elevated in cells expressing Pex13p-KRNT grown under the same
conditions (Fig. 5A & B). To assess whether the increased levels of Pex13-KRNT stem
from an inhibition in degradation, we followed Pex13-KRNT turnover in CHX treated
cells, observing that Pex13-KRNT degradation was indeed slower than that of the WT
protein (Fig. 6), although we note that degradation was not completely blocked. Taken
together, our data demonstrate that blocking NH2 groups in Pex13p inhibit its rapid
degradation.
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Fig. 4 Pex13p degradation is not inhibited in H. polymorpha Pex13 (Δpest) cells.
A Schematic diagram of H. polymorpha Pex13p, showing the position of the putative
PEST sequence (DNNA TTST DNSS APPE LPT). TM depicts transmembrane domains
while SH3 depicts the SH3 domain in Pex13p.
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B WT cells expressing Pex13-His6 were grown on methanol/glycerol media for 12 hrs and
treated with DMSO (Ctrl) or Cycloheximide (CHX). TCA samples were taken at the
indicated time (hrs) after DMSO/CHX addition and probed by SDS-PAGE and
immunoblotting with antibodies against His6-tag, Pex14p, Pex11p and Pyc.
C Representative western blots of samples from Pex13-His6(Δpest) cells grown and
treated as in A. Samples were probed with SDS-PAGE and immunoblotting with
antibodies against His6-tag, Pex11p and Pyc.
D Quantification of Pex13-His6 levels in WT and Pex13 (Δpest) cells. Protein levels were
normalized to the loading control Pyc at the corresponding time point. Protein levels at
T0 were set to 1. Values represent the mean ± SD of three independent experiments.
E Quantification of Pex14p and Pex11p levels in WT and Pex13 (Δpest) cells. Protein
levels were normalized to Pyc at the corresponding time point. Protein levels at T0 were
set to 1. Values represent the mean ± SD of three independent experiments.
Fig. 5 Blocking NH2 groups in Pex13p results in enhanced protein levels.
A Representative western blots of samples derived from WT and mutant cells grown for 16
hrs on methanol/glycerol media. Blots were probed with antibodies directed against the
His6-tag, Pex14p, Pex11p and Pyc.
B Quantification of protein in WT and mutant cells, normalized to the loading control Pyc
at the corresponding time point. Protein levels in WT cells were set to 1. Values
represent the mean ± SD of three independent experiments. An asterisks denotes
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statistically significant increases in protein levels compared to those in WT samples
(**P < 0.01).
Inhibiting Pex13p degradation reduces cell growth on methanol containing media
To investigate whether inhibiting Pex13p degradation affected the function of the
protein, we assessed the ability of cells expressing Pex13-KRNT to grow on methanol
containing media. Note that all versions of Pex13p used in these growth assays
contained a His6-tag, allowing direct comparisons. Growth was assessed by measuring
the optical density at 600nm (OD600) of cultures grown on methanol media and
methanol/ glycerol media after 16 hours. Cells expressing Pex13-KRNT, under control
of the endogenous PEX13 promoter, did not display a growth defect when grown on
media containing methanol as sole carbon source (Fig. 7A). Both strains also grew
comparably well on methanol media containing glycerol (Fig. 7A). At first glance, these
data could suggest that inhibiting Pex13p degradation does not affect peroxisome
function. However, we suspected that overproduction of Pex13-KRNT may prove more
successful for two reasons: (1) we noted that Pex13p degradation was reduced but not
completely abolished by the KRNT mutations (Fig. 6A-C) and (2) we deemed it
possible that the amount of Pex13p in cells expressing Pex13-KRNT under control of
the PEX13 promoter may not have reached a critical point. Therefore, we made
constructs in which His6-tagged Pex13 or Pex13-KRNT was under control of the strong
AOX promoter and we assessed the growth of these cells on methanol and methanol/
glycerol media. Our data indicate that overproduction of WT Pex13-His6 reduces the
ability of cells to grow on both types of media (Fig. 7A), an observation that is
consistent with previous work in S. cerevisiae (Bottger et al, 2000). However, we also
observed that the growth of cells overproducing Pex13-KRNT was consistently poorer
than that of cells overproducing WT Pex13-His6 (Fig 7A). Western blotting analysis
confirmed that Pex13-His was overproduced in both strains (Fig. 7B). To investigate
further the effect of overproducing Pex13-His6 on cell growth, we performed growth
curve experiments (Fig. 7C & D), confirming that cells overproducing Pex13-KRNT
display a slower growth rate than those overproducing WT Pex13-His6.
Pex13p degradation exhibits a synergistic relationship with Pex14p levels
Overproduction of either Pex13p or Pex14p inhibits peroxisome function in both S.
cerevisiae (Bottger et al, 2000) and H. polymorpha (Fig. 7 and (Komori et al, 1997))
whereas co-overproduction of Pex13p and Pex14p in S. cerevisiae does not (Bottger et
Further insights into Pex13p degradation THREE
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al, 2000), indicating that the balance between Pex13p and Pex14p levels are important
for peroxisome function. However, we observed that Pex14p levels are largely
unaffected by either deletion or overexpression of PEX13 (Fig. 3 and (Chen et al, 2018)),
whereas Pex13p levels are increased in cells deleted for PEX14 (Fig. 3 and (Chen et al,
2018)). Taken together, these data could suggest that the level of Pex13p depends on that
of Pex14p, rather than vice versa. In this assumption, the degradation of Pex13p would
undergo a correlative change in cells overproducing Pex14p. Therefore, we determined
Pex13p levels in cells expressing Pex14p under control of AMO promoter grown on
methanol/ glycerol media. Pex13p levels were increased in cells overproducing Pex14p
(Fig. 8), suggesting that Pex13p degradation is reduced in these cells and that Pex13p
degradation is dependent on Pex14p levels. Together, these results identify a synergistic
relationship between Pex13p degradation and Pex14p levels.
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Fig. 6 Pex13p with blocked NH2 groups displays a reduced turnover.
A WT cells expressing Pex13-His6 were grown on methanol/glycerol media for 12 hrs and
treated with DMSO (Ctrl) or Cycloheximide (CHX). TCA samples were taken at the
indicated time (min) after DMSO/CHX addition and probed by SDS-PAGE and
immunoblotting with antibodies against His6-tag, Pex14p, Pex11p and Pyc.
B Representative western blots of samples derived from cells grown and treated as in A
expressing His6-tagged Pex13-KRNT. Samples were probed with SDS-PAGE and
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immunoblotting with antibodies against His6-tag, Pex14p, Pex11p and Pyc.
C Quantification of His6-tagged Pex13 levels in WT and Pex13-KRNT cells. Protein
levels were normalized to the loading control Pyc at the corresponding time point.
Protein levels at T0 were set to 1. Values represent the mean ± SD of three independent
experiments (*P < 0.05).
D Quantification of Pex14p and Pex11p levels in WT and Pex13-KRNT cells. Protein
levels were normalized to Pyc at the corresponding time point. Protein levels at T0 were
set to 1. Values represent the mean ± SD of three independent experiments.
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Fig. 7 Overproduction of Pex13-KRNT impacts on the ability of cells to grown on
methanol containing media.
A OD600 measurements of cells grown on methanol or methanol/ glycerol media for 16 hrs.
Cells were grown on glucose to exponential phase before shifting to methanol mineral
medium. Values represent the mean ± SD of two independent experiments. An asterisks
denotes a statistically significant difference in the OD value (*P < 0.05, **P < 0.01,
***P < 0.001) compared to that of the WT strain (above the column) or between the
Paox-Pex13 and Paox-Pex13-KRNT strains (indicated with a line).
B Confirmation of Pex13p overproduction. Representative western blots of samples
derived cells grown for 16 hrs on methanol/ glycerol media. Blots were probed with
antibodies directed against the His6-tag, Pex14p, Pex11p and Pyc. L.E. stands for long
exposure.
C Growth curve of cells grown on methanol (left panel) or methanol/glycerol (right panel)
media over a 16 hour period. Cells were grown on glucose to exponential phase before
shifting to methanol containing media.
Fig. 8 Pex13p levels exhibit a synergistic increase with Pex14p overexpression.
A Representative western blots of samples derived cells grown for 16 hrs on methanol/
glycerol media. Blots were probed with antibodies directed against Pex13p, Pex14p,
Pex11p and Pyc.
B Quantification of protein levels in WT and mutant cells, normalized to the loading
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control Pyc at the corresponding time point. Protein levels in WT cells were set to 1.
Values represent the mean ± SD of three independent experiments. An asterisks denotes
statistically significant increases in protein levels compared to those in WT samples
(*P<0.05, **P < 0.01).
Discussion
At some point during their lifetime, all the proteins in a cell will undergo protein
degradation. This may be because they are “worn out” by chemical modifications,
because they become unfolded or because they are no longer needed. Protein
degradation needs to be regulated, otherwise unwanted degradation events may occur or
unwanted proteins start to build up in the cell. Hence, understanding how and why
proteins are degraded allows us to better understand the role of protein degradation in a
cellular context.
The PMP Pex13p is a member of the peroxisomal docking complex and it plays an
essential role in the import of PTS1 and PTS2 containing proteins into peroxisomes.
Previously we demonstrated that Pex13p undergoes UPS-mediated degradation in the
yeast H. polymorpha (Chen et al, 2018). Here, we have investigated further the Pex13p
degradation event in H. polymorpha. We provide evidence that Pex5p recycling is linked
to Pex13p degradation. Pex5p shuttles between the cytosol and the peroxisomal
membrane and its recycling from the membrane requires Pex5p to be
mono-ubiquitinated (Platta et al, 2007). When Pex5p mono-ubiquitination is inhibited
(through mutation of the conserved cysteine in Pex5p or in pex4 cells), Pex5p is
degraded (Kiel et al, 2005b; Leon & Subramani, 2007). The level of Pex13p was
increased in cells where the recycling of Pex5p was inhibited (Pex5-C9S mutant), while
the levels of Pex13p were even more elevated in cells where both Pex5p recycling and
degradation were blocked (Pex5-C9S.K21R and pex4 cells expressing Pex5-K21R). In
this mutant, Pex5p cannot be mono- or poly-ubiquitinated (Kiel et al, 2005b; Williams et
al, 2007), leading to a buildup of Pex5p on the peroxisomal membrane (Platta et al,
2007). One possible explanation for our data is that Pex5p removal from the membrane
is coupled to Pex13p degradation and that maybe both proteins can leave the
peroxisomal membrane together. An alternative theory is that Pex5-C9S.K21R simply
blocks the interaction between Pex13p and the counterpart proteins required for its
ubiquitination/degradation. However, we note here that although our data establish a
link between Pex5p recycling and Pex13p degradation, inhibiting Pex5p recycling also
blocks PTS1 protein import (Williams et al, 2007), meaning that we cannot rule out that
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the increased levels of Pex13p in the Pex5-C9S.K21R mutant stem from a decrease in
PTS1 protein import. In addition, levels are increased in pex14 and pex5 cells (Chen et
al, 2018), suggesting that Pex13p degradation requires a fully functional matrix import
pathway. Therefore, further study into the role of Pex5p cycling in Pex13p degradation
is required.
Blocking all the NH2 groups in Pex13p, the likely sites of Pex13p ubiquitination,
results in elevated Pex13p levels and a reduced turnover rate. However, we note that the
degradation of Pex13p is not completely inhibited by these mutations (see Fig. 6),
leaving the question of how this may be facilitated? In the absence of NH2 groups, it is
possible that Pex13p ubiquitination may occur on additional residues, such as serine,
threonine or cysteine residues. Ubiquitination of these residues has been reported (Wang
et al, 2007; Williams et al, 2007). This would allow Pex13p degradation to still occur,
although this may occur at a reduced rate, explaining the effect of the Pex13-KRNT
mutant. Alternatively, certain substrates of the proteasome can be recognized and
degraded without a prior need to be ubiquitinated (Sheaff et al, 2000; Shringarpure et al,
2003), which could suggest that Pex13p is still degraded even though it cannot be
ubiquitinated efficiently. Gaining information on the ubiquitination status of
Pex13-KRNT will shed light on this.
Overproduction of WT Pex13p results in reduced cell growth on methanol media,
likely because of a blockage to matrix protein import. Interestingly, this phenotype is
enhanced in cells overproducing Pex13-KRNT, suggesting that inhibiting Pex13p
degradation in these cells impacted negatively on peroxisome function. However, no
growth defect was seen with cells producing Pex13-KRNT under the control of the
endogenous PEX13 promoter. This presents a model in which a critical level of Pex13p
exists and if Pex13p levels stay under this point, peroxisome function can occur
normally. If Pex13p levels go above this point, peroxisome function is disturbed.
Comparably, cells overexpressing PEX14 from the AOX promoter display a matrix
protein import defect whereas peroxisomes in cells overexpressing PEX14 from the
weaker amine oxidase (AMO) promoter are still able to import matrix proteins (Komori
et al, 1997). Hence, our data suggest that the degradation of Pex13p in cells
overproducing Pex13p countered, to a certain extent, the detrimental effects of Pex13p
overproduction, indicating that the ability to degrade Pex13p can be an asset.
Our latest results, together with our previous report (Chen et al, 2018), demonstrate
that Pex13p degradation occurs in cells grown both on glucose and methanol containing
media. In addition, degradation under both growth conditions requires a functional
peroxisomal E3 ligase complex. Together, our data establish that Pex13p degradation is
Further insights into Pex13p degradation THREE
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a general process and not a condition specific one, indicating that rather than a quality
control mechanism that removes faulty proteins, Pex13p degradation is more likely to be
a targeted degradation event. Comparably, we previously reported that degradation of
the PMP Pex3p is required before peroxisomes undergo autophagic degradation
(Williams & van der Klei, 2013b). So, what could the function of Pex13p degradation be?
Pex13p is constitutively degraded while its binding partner Pex14p is more stable (see
Fig. 1 and (Chen et al, 2018)). These data suggest that the levels of these two proteins
are regulated differently. Hence, Pex13p may harbour a degron-like signal to mediate its
degradation yet the putative PEST sequence in the N-terminal region appears not to be
involved in Pex13p turnover (Fig. 4). However, our data suggest that Pex14p levels play
a determining role in Pex13p degradation (Fig. 8) yet varying Pex13p levels have little
or no effect on Pex14p levels (Fig. 7 and (Chen et al, 2018)). This, coupled with the fact
that overproduction of Pex13p and Pex14p together has no effect on the ability of S.
cerevisiae cells to grow on oleate-containing media (Bottger et al, 2000), could suggest
that Pex13p levels (and hence Pex13p degradation) are regulated depending on those of
its binding partner Pex14p. While Pex14p complexes lacking Pex13p have been isolated
from cells (Meinecke et al, 2010), we suspect that a large portion of Pex14p will be
bound to Pex13p at any one time, because of the many different interactions these
proteins have with each other (Girzalsky et al, 1999; Schell-Steven et al, 2005). In this
respect, perhaps Pex13p degradation represents a way in which excess Pex13p that is
not bound to Pex14p can be removed from the cell. Inhibiting Pex13p degradation can
impact negatively on peroxisome function (Fig. 7). However, if an important part of
Pex13p function is to keep Pex14p in complex, why degrade Pex13p in the first place?
Blocking Pex13p degradation did not impact on peroxisome function when Pex13p was
not overproduced (Fig. 7), suggesting that the cell can handle a modest increase in
Pex13p levels. Therefore, we suspect that the removal of excess Pex13p from the
peroxisomal membrane is a plausible reason for why Pex13p is degraded, but we also
consider it likely that the rapid degradation of Pex13p may serve several purposes.
Following on from this, perhaps Pex13p degradation could also serve to negatively
regulate matrix protein import. Pan et al proposed a similar theory, based on their data
on Pex13p degradation in plants (Pan et al, 2016). Rapid degradation of Pex13p could
disconnect the docking complex from the downstream components required for PTS1
protein import, such as the RING E3 complex or the AAA-ATPases Pex1p and Pex6p,
which would undoubtedly inhibit PTS1 protein import. Such negative regulation of
import could be relevant in fully grown or mature peroxisomes because it can be
imagined that such peroxisomes need to import way less matrix proteins (Kumar et al,
THREE Further insights into Pex13p degradation
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2017; Legakis et al, 2002). Indeed, Pex13p levels are dynamic over time, peaking at
around 6-8 hours in cells grown on methanol/ glycerol containing media and then
declining at later time-points (Knoops et al, 2014), which may suggest that Pex13p is
surplus to requirements at later stages of cell growth.
However, Pex13p degradation is a rapid and general event, which might not be
explained by the notion of negative regulation of matrix protein import. This, coupled
with the observation that Pex13p degradation is linked to Pex5p recycling, could suggest
that Pex13p degradation may instead positively regulate PTS1 protein import. A possible
function for Pex13p degradation may be to dissociate the importomer complex. The
importomer is a transient protein complex at the peroxisomal membrane, consisting of
the docking complex (Pex13p, Pex14p and Pex17p), the receptor plus cargo and proteins
involved in Pex5p recycling (RING E3 ligases, Pex1p, Pex6p and Pex15p) (Oeljeklaus
et al, 2012). The importomer forms after docking of the receptor-cargo complex on the
peroxisomal membrane and is required for transport of matrix proteins into the
peroxisomal lumen (Deckers et al, 2010; Meinecke et al, 2010; Oeljeklaus et al, 2012).
Because of the transient nature of the importomer complex, it could be envisaged that
removal of Pex13p out of the importomer complex may destabilize the importomer and
lead to the release of cargo proteins into the lumen or alternatively to the recycling
Pex5p to the cytosol. Such a model would fit with a role for Pex13p in the cargo
translocation or receptor recycling steps of matrix protein import, as was previously
suggested (Williams & Distel, 2006). Furthermore, we demonstrated that blocking
Pex13p degradation can impact on cell growth (Fig. 7), which would support a model
where Pex13p degradation regulated PTS1 protein import in a positive manner. Hence,
further work that addresses the role of Pex13p degradation in matrix protein import is
required.
Finally, while the function of Pex13p degradation remains unclear, we note that
Pex13p in the yeast S. cerevisiae is also degraded via the UPS (see Chapter 4 of this
thesis). Furthermore, Pan et al demonstrated that Pex13p in plants undergoes
UPS-mediated degradation (Pan et al, 2016), although the mechanisms that facilitate this
degradation event remain controversial (Ling et al, 2017; Pan & Hu, 2018). Therefore,
Pex13p degradation occurs in at least three different organisms, demonstrating that it is a
conserved process and we anticipate that the regulated degradation of Pex13p is a
fundamental property of peroxisomes.
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93
Materials and Methods
Molecular techniques and construction of H. polymorpha strains
Transformation of H. polymorpha was performed by electroporation, as described
previously (Faber et al, 1994). H. polymorpha strains used in this study are listed in
Table 1. The plasmids and primers used in this study are listed in Table 2 and 3
respectively. Phusion DNA polymerase (Thermo Scientific) was used to produce gene
fragments.
The pHIPZ-Pex13-mGFP plasmid (Knoops et al, 2014) was linearized with ApaI
prior to transformation into H. polymorpha cells. pHIPH-Pex14-mKate2 (Chen et al,
2018) was linearized with Bpu1102I prior to transformation into H. polymorpha cells.
Plasmids containing the PEX13 promoter (see below) were linearized with NheI prior to
transformation into H. polymorpha cells.
To construct pHIPZ20-Pex13(K-R)-His6, a synthetic gene fragment of PEX13 with
all lysine coding sequences changed to arginine coding sequences was ordered from
BaseClear (Leiden, The Netherlands). PCR was performed on this gene fragment using
primers SalI-P13R-F and P13R-His6-XbaI-R, and the resulting Pex13(K-R)-His6 DNA
fragment was digested with SalI and XbaI and ligated into SalI-XbaI digested
pHIPZ20-mGFP (Chen et al, 2018), producing pHIPZ20-Pex13(K-R)- His6.
The plasmid pHIPZ20-Pex13(Δpest)-His6 was constructed as follows: A fragment
of 240 bp of Pex13, without the region encoding for the putative PEST sequence (amino
acids 25-43) and containing SalI and NdeI sites was obtained from Integrated DNA
Technologies (https://eu.idtdna.com/pages/home). The fragment was digested with SalI
and NdeI and ligated into SalI-NdeI digested pHIPZ20-Pex13- His6 (Chen et al, 2018),
producing pHIPZ20-Pex13(Δpest)-His6.
The plasmid pHIPZ20-MSE-His6-Pex13 was constructed by PCR on the plasmid
pHIPZ20-Pex13-His6 (Chen et al, 2018) using primers SalI-His6-Pex13-F and
Pex13-XbaI-R, and the resulting MSE-His6-Pex13 fragment was digested with SalI and
XbaI and cloned into pHIPZ20-Pex13-His6 between SalI and XbaI sites.
Plasmid pHIPZ20-MSE-His6-Pex13(K-R) was constructed as follows: PCR was
performed on the plasmid pHIPZ20-Pex13(K-R)-His6 using primers
SalI-His6-Pex13(K-R)-F and Pex13R-XhoI-R, and the resulting MSE-His6-Pex13(K-R)
fragment was digested with SalI and XhoI and cloned into pHIPZ20-Pex13-His6
between SalI and XhoI sites.
To construct plasmid pHIPZ4-Pex13-His6, PCR was performed on the plasmid
pHIPX4 (Gietl et al, 1994) using primers NotI-Paox-F and Paox-SalI-R, and the
resulting AOX promoter was digested with NotI and SalI and cloned into
THREE Further insights into Pex13p degradation
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pHIPZ20-Pex13-His6 between NotI and SalI sites. The construct
pHIPZ4-MSE-His6-Pex13-(K-R) was made in similar way. Plasmids containing the
AOX promoter were linearized with Ppu10I prior to transformation into H. polymorpha
cells.
To construct pHIPZ12-Pex5-C9S, a 596 bp PCR fragment consisting of the PEX5
promoter and the 5’ end of PEX5, introducing the C9S mutation, was first produced by
PCR using pRBG56-2 (Kiel et al, 2005b) as template and with primers Universal
M13/pUC and Pex5-C9S-R. The resulting DNA fragment was used as forward primer,
together with primer Pex5-return, and pRBG56-2 as template to produce a fragment
harbouring an XhoI restriction site. This 754 bp fragment was then cloned into
pHIPX4-Pex5 (Van der Klei et al, 1995) between NotI and XhoI. The product was
digested with NotI and NheI and the PEX5 containing fragment of 3156 bp was cloned
into pHIPZ4 (Salomons et al, 2000) between NotI and XbaI. The
pHIPZ12-Pex5-C9S.K21R plasmid was produced in the same manner as described but
instead pHIPZ12-Pex5-K21R was used as template. Plasmids containing the PEX5
promoter were linearized with BsiWI prior to transformation into H. polymorpha cells.
All integrations were confirmed by colony PCR using Phire Hot Start II (Thermo
Scientific) and strains containing Pex13(K-R)-His6, Pex13(Δpest)-His6, Pex13-NT,
Pex13-KRNT, Pex5-C9S or Pex5-C9S.K21R were further checked with Southern
blotting.
Southern blotting
Southern blotting analysis was performed using the ECL Direct Nucleic Acid Labelling
and Detection system (Thermo Scientific) according to the established methods. H.
polymorpha genomic DNA containing the integrated pHIPZ20-based plasmids was
digested with EcoRI (Thermo Scientific). The probe for Pex13(K-R)-His6, consisting of
a 0.5 kb fragment 1 kb-upstream, was amplified using primers Sthn-13(R)CSProbF and
Sthn-13(R)CSProbR. The probe recognises a 2.5 kb fragment in pex13 cells and an ~8
kb fragment in one-copy mutant cells.
H. polymorpha genomic DNA containing the integrated pHIPZ12-Pex5-C9S or
pHIPZ12-Pex5-C9S.K21R plasmid was digested with HindIII (Thermo Scientific). The
probe for Pex5-C9S or Pex5-C9S.K21R, consisting of a 0.5 kb fragment 1kb-upstream,
was amplified using primers Sthn-d5-Probe-F and Sthn-d5-Probe-R. The probe
recognizes a 2.5 kb fragment in pex5 cells and a ~10 kb fragment in one-copy mutant
cells.
Further insights into Pex13p degradation THREE
95
Prediction of PEST sequence in Pex13p
The full-length H. polymorpha Pex13p sequence was obtained from the NCBI website
(https://www.ncbi.nlm.nih.gov/gene/25771723) and the program epestfind
(http://emboss.bioinformatics.nl/cgi-bin/emboss/epestfind) was used to search the
sequence for putative PEST sequences. A putative PEST sequence
(DNNATTSTDNSSAPPELPT) was found between residues NSLDK and RPSSL,
displaying a score of 13.1. PEST motifs below the threshold score (5.0) are considered
as poor, while PEST scores above the threshold are considered significant.
Prediction of N-terminal acetylation
The sequence of the first ten amino acids at the N-terminus of H.polymorpha Pex13p is
MTTPRPKPWE, which is not predicted to be acetylated, according to NetAcet
(http://www.cbs.dtu.dk/services/NetAcet/). To inhibit the potential ubiquitination of NH2
group at the N-terminus, we made a mutant version of Pex13p that was predicted to be
acetylated (Kiemer et al, 2004). To achieve this, we added a sequence encoding for
serine and glutamic acid after the start codon (MSE), followed by a sequence encoding
for a 6*His tag and then the full-length PEX13. The resulting amino sequence (MSEHH)
was predicted to be acetylated using NetAcet (http://www.cbs.dtu.dk/services/NetAcet/).
Strains and growth conditions
Yeast transformants were selected on YPD plates containing 2% agar and 100 μg/ml
Zeocin (Invitrogen) or 300 μg/ml Hygromycin (Invitrogen). The E. coli strain DH5α
was used for cloning purposes. E. coli cells were grown in LB supplemented with
100 μg/ml Ampicillin at 37 °C. H. polymorpha cells were grown in batch cultures at
37 °C on mineral media supplemented with 0.25% glucose or 0.5% methanol (either
with or without 0.05% glycerol) as carbon source and 0.25% ammonium sulphate or
0.25% methylamine as nitrogen source. Leucine, when required, was added to a final
concentration of 30 μg/ml. Cycloheximide (CHX) when used, was added to a final
concentration of 6 mg/ml.
Preparation of yeasts TCA lysates
Cell extracts of TCA-treated cells were prepared for SDS-PAGE as detailed previously
(Baerends et al, 2000). Equal amounts of protein were loaded per lane and blots were
probed with rabbit polyclonal antisera raised against the Myc tag (Santa Cruz Biotech,
sc-789), Pex5p (Kiel et al, 2005b), Pex13p (Chen et al, 2018), Pex14p (Komori et al,
1997), Pex11p (Knoops et al, 2014) or pyruvate carboxylase 1 (Pyc1) (Fahimi et al,
THREE Further insights into Pex13p degradation
96
1993) or mouse monoclonal antisera raised against penta-His tag (Qiagen, 34660) or
mGFP (Santa Cruz Biotech, sc-9996). Secondary goat anti-rabbit (31460) or goat
anti-mouse (31430) antibodies conjugated to horseradish peroxidase (Thermo Fisher
Scientific) were used for detection. Pyc1 was used as a loading control. Note that the
anti-Pex14p can recognise both the phosphorylated (upper band) and unphosphorylated
(lower band) forms of Pex14p.
Quantification of Western blots
Blots were scanned by using a densitometer (GS-710; Bio-Rad Laboratories) and
protein levels were quantified using Image Studio Lite Ver5.2 software (LI-COR
Biosciences). In the case of Pex14p blots, both the phosphorylated and
unphosphorylated forms were included in the calculation if both forms were visible. The
value obtained for each band was normalized by dividing it by the value of the
corresponding Pyc band (loading control). For comparison of absolute protein levels
(Figures 1, 3 and 5), normalized values obtained for Pex13p, Pex14p and Pex11p levels
in WT cells were set to 1 and the levels of these proteins in mutant cells are displayed
relative to WT. For CHX experiments (Figures 2, 4 and 6), the normalized values of T0
samples were set to 1.0 and values obtained from the T1-T3 samples are displayed as a
fraction of T0 values. Standard deviations and significance were calculated using Excel.
* represents P-values < 0.05, ** represents P-values < 0.01 and *** represents P-values
< 0.001. The data presented are derived from three independent experiments.
Fluorescence Microscopy
All fluorescence microscopy images were acquired using a 100×1.30 NA Plan-Neofluar
objective (Carl Zeiss). Wide-field microscopy images were captured by an inverted
microscope (Axio Scope A1, Carl Zeiss) using Micro-Manager software and a digital
camera (CoolSNAP HQ2; Photometrics). GFP signal was visualized with a 470/440-nm
band pass excitation filter, a 495-nm dichromatic mirror, and 525/550-nm band pass
emission filter.
For images taken of Pex13-mGFP in WT grown on glucose mineral medium, the
optimal settings were mGFP (255, 800) and mKate2 (219, 1200), and in pex2, the
optimal settings mGFP (255, 3000) and mKate2 (219, 2200) were applied for processing.
The general settings used to compare the signal of Pex13-mGFP in WT and pex2, mGFP
(255, 2000) and mKate2 (219, 1700) were applied for processing.
For quantification of the Pex13-mGFP signal in WT or pex2 cells, a rectangular
area was drawn using the “rectangular tool” from ImageJ (Abramoff et al, 2004) to
Further insights into Pex13p degradation THREE
97
envelope the region containing the Pex13-mGFP spot and pixel intensity inside the area
was measured. The measured maximum fluorescence intensity of GFP on peroxisomes
was corrected for the background intensity and a box plot was made using Microsoft
Excel. The box represents values from the 25 percentile to the 75 percentile; the
horizontal line through the box represents the median value. Whiskers indicate
maximum and minimum values.
Acknowledgements
The authors thank Thomas Schroeter, Jessica Kluemper, Wolfgang Schliebs and Ralf
Erdmann for helpful discussions and Arjen Krikken for advice with processing of
fluorescence microscopy images. This work was funded by a VIDI Fellowship
(723.013.004) from the Netherlands Organisation for Scientific Research (NWO),
awarded to CW.
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Table 1, H. polymorpha strains used in this study
Strain Description Reference
WT Hp WT (NCYC495), leu1.1 (Gleeson &
Sudbery,
1988)
WT Pex13-mGFP Hp WT with pHIPZ-Pex13-mGFP (zeoR),
leu1.1
(Chen et al,
2018)
pex2 pex2 disruption strain, leu1.1 (Koek et al,
2007)
pex2+ Pex13-mGFP pex2 with pHIPZ-Pex13-mGFP (zeoR), leu1.1 (Chen et al,
2018)
pex2+ Pex13-mGFP+
Pex14-mKate2
pex2 with pHIPZ-Pex13-mGFP (zeoR) and
pHIPH-Pex14-mKate2 (hygR), leu1.1
(Chen et al,
2018)
pex4 pex4 disruption strain, leu1.1 (Van der
Klei et al,
1998)
pex4+ Pex13-mGFP pex4 with pHIPZ-Pex13-mGFP (zeoR), leu1.1 This study
pex4+ Pex13-mGFP+
Pex14-mKate2
pex4 with pHIPZ-Pex13-mGFP (zeoR) and
pHIPH-Pex14-mKate2 (hygR), leu1.1
This study
pex13 pex13 disruption strain, leu1.1 (Koek et al,
2007)
pex14 pex14 disruption strain, leu1.1 (Komori et
al, 1997)
Pex5-C9S pex5 with one copy of plasmid
pHIPZ12-Pex5-C9S (zeoR) integrated
This study
Pex5-K21R pex5 with one copy of plasmid
pHIPZ12-Pex5-K21R (zeoR) integrated
(Kiel et al,
2005b)
Pex5-C9S.K21R pex5 with one copy of plasmid
pHIPZ12-Pex5-C9S.K21R (zeoR) integrated
This study
pex4+ Pex5-K21R pex4 with one copy of plasmid
pHIPZ12-Pex5-K21R (zeoR) integrated
This study
pex5 pex5 disruption strain, leu1.1 (Van der
Klei et al,
1995)
Pex13-His6 pex13 with one copy of plasmid (Chen et al,
Further insights into Pex13p degradation THREE
99
pHIPZ20-Pex13-His6 (zeoR), leu1.1 2018)
Pex13(Δpest)-His6 pex13 with one copy of plasmid
pHIPZ20-Pex13(Δpest)-His6 (zeoR), leu1.1
This study
Pex13-KR-His6 pex13 with one copy of plasmid
pHIPZ20-Pex13(K-R)-His6 (zeoR), leu1.1
This study
Pex13-NT-His6 pex13 with one copy of plasmid
pHIPZ20-MSE-His6-Pex13 (zeoR), leu1.1
This study
Pex13-KRNT-His6 pex13 with one copy of plasmid
pHIPZ20-MSE-His6-Pex13(K-R) (zeoR),
leu1.1
This study
Paox-Pex13-His6 pex13 with one copy of plasmid
pHIPZ4-Pex13-His6 (zeoR), leu1.1, under
control of AOX promoter
This study
Paox-Pex13-KRNT-
His6
pex13 with one copy of plasmid
pHIPZ4-MSE-His6-Pex13(K-R) (zeoR),
leu1.1, under control of AOX promoter
This study
Table 2, plasmids used in this study
Plasmid Description Reference
pHIPZ-Pex13-mGFP C-terminal part of PEX13 fused with
mGFP, zeoR
; ampR
(Knoops et
al, 2014)
pHIPH-Pex14-mKate2 Plasmid containing the C-terminal
region of PEX14 fused to mKate2;
hygR
; ampR
(Chen et al,
2018)
pHIPZ20-mGFP mGFP under control of PEX13
promoter, zeoR
; ampR
(Chen et al,
2018)
pHIPZ12-Pex5-C9S Plasmid containing Pex5 in which the
Cysteine-9 was changed to Serine
residue, under control of PEX5
promoter, zeoR, kan
R
This study
pHIPZ12-Pex5-K21R Plasmid containing Pex5 with the
Lysine-21 changed to Arginine, under
control of PEX5 promoter, zeoR, kan
R
(Kiel et al,
2005b)
pHIPZ12-Pex5-C9S.K21R Plasmid containing Pex5 with the This study
THREE Further insights into Pex13p degradation
100
Cysteine-9 changed to Serine residue
and Lysine-21 to Arginine, under
control of PEX5 promoter, zeoR, kan
R
pHIPZ20-Pex13-His6 Pex13 fused to a 6*His tag at its
C-terminus, under control of PEX13
promoter, zeoR
; ampR
(Chen et al,
2018)
pHIPZ20-Pex13(K-R)-His6 Pex13 with all lysine residues
changed to arginine ones fused to a
6*His tag at its C-terminus, under
control of PEX13 promoter, zeoR
;
ampR
This study
pHIPZ0-Pex13(Δpest)-His6 Pex13 without PEST sequence fused
to a 6*His tag at its C-terminus, under
control of PEX13 promoter, zeoR;
ampR
This study
pHIPZ20-MSE-His6-Pex13 Pex13 fused to MSE and a 6*His tag
at its N-terminus, under control of
PEX13 promoter, zeoR; amp
R; also
written as (Pp13-)Pex13-NT
This study
pHIPZ20-MSE-His6-Pex13(K-R) Pex13 with all lysine residues
changed to arginine ones fused to
MSE and a 6*His tag at its
N-terminus, under control of PEX13
promoter, zeoR; amp
R; also written as
(Pp13-)Pex13-KRNT
This study
pHIPX4 Plasmid with H. polymorpha
AOX promoter and AMO terminator;
kanR, ScLEU2
(Gietl et al,
1994)
pHIPZ4-Pex13-His6 Pex13 fused to a 6*His tag at its
C-terminus, under control of AOX
promoter, zeoR
; ampR
This study
pHIPZ4-MSE-His6-Pex13(K-R) Pex13 with all lysine residues
changed to arginine ones fused to
MSE and a 6*His tag at its
N-terminus, under control of AOX
promoter, zeoR; amp
R; also written as
This study
Further insights into Pex13p degradation THREE
101
Paox-Pex13-KRNT
Table 3, primers used in this study
Primer Sequence Description
SalI-P13-F ACGCGTCGACATGACTACA
CCACGTCCAAAG
To clone the Pex13 gene,
forward primer, used to make
construct
pHIPZ20-Pex13(Δpest)-His6
SalI-P13R-F ACGCGTCGACATGACTACA
CCACGTCCACG
To clone the Pex13(K-R) gene,
forward primer, used to make
construct
pHIPZ20-Pex13(K-R)-His6
P13-His6-XbaI-R CTAGTCTAGATCAGTGATG
GTGATGGTGATGGATCAAA
AGCTTTTGATCTTTCTTG
To clone the Pex13 gene with
His*6 tag, reverse primer, used
to make construct
pHIPZ20-Pex13-His6
P13R-His6-XbaI-
R
CTAGTCTAGATCAGTGATG
GTGATGGTGATGGATCAAA
AGACGTTGATCACG
To clone the Pex13(K-R) gene
with His*6 tag on its C-terminus,
reverse primer, used to make
construct
pHIPZ20-Pex13(K-R)-His6
SalI-His6-Pex13(
K-R)-F
ACGCGTCGACATGAGTGAA
CATCACCATCACCATCACA
CTACACCACGTCCACGTC
To clone the Pex13(K-R) gene
fused to M (the start codon
ATG)-SE and His*6 tag at its
N-terminus, forward primer, used
to make construct
pHIPZ20-MSE-His6-Pex13(K-R
) and
pHIPZ4-MSE-His6-Pex13(K-R)
Pex13R-XhoI-R GGCCTCGAGTCAGATCAAA
AGACGTTGATCAC
To clone the Pex13(K-R) gene,
reverse primer, used to make
construct
pHIPZ20-MSE-His6-Pex13(K-R
) and
THREE Further insights into Pex13p degradation
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pHIPZ4-MSE-His6-Pex13(K-R)
NotI-Paox-F ATAAGAATGCGGCCGCTCG
ACGCGGAGAACG
To clone the AOX promoter,
forward primer, used to make
construct pHIPZ4- Pex13-His6
and
pHIPZ4-MSE-His6-Pex13(K-R)
Paox-SalI-R ACGCGTCGACGTTTTTGTAC
TTTAGATTGATGTCACCACC
To clone the AOX promoter,
reverse primer, used to make
construct pHIPZ4- Pex13-His6
and
pHIPZ4-MSE-His6-Pex13(K-R)
SalI-His6-Pex13-
F
ACGCGTCGACATGAGTGAA
CATCACCATCACCATCACA
CTACACCACGTCCAAAGC
To clone the Pex13 gene fused to
M (the start codon ATG)-SE and
His*6 tag at its N-terminus,
forward primer, used to make
construct
pHIPZ20-MSE-His6-Pex13
Pex13-XbaI-R CTAGTCTAGATCAGATCAA
AAGCTTTTGATCTTTC
To clone the Pex13 gene, reverse
primer, used to make construct
pHIPZ20-MSE-His6-Pex13
Sthn-13(R)CSPro
bF
CAACAACGAATCTAGATTC
AAGAC
To clone the probe for
Pex13*-His Southern blotting,
forward primer
Sthn-13(R)CSPro
bR
TCGTTACCTGTGATGCTACA
G
To clone the probe for
Pex13*-His Southern blotting,
reverse primer
Sthn-d5-Probe-F AGCAAAGACGAAAGGTGC To clone the probe for Pex5
mutants Southern blotting,
forward primer
Sthn-d5-Probe-R CACAAACATGTATAAGATG
ACCAG
To clone the probe for Pex5
mutants Southern blotting,
reverse primer
Universal
M13/pUC
GTTTTCCCAGTCACGAC To clone a 596 bp PCR fragment
consisting of the PEX5 promoter
and the 5’ end of PEX5,
introducing the C9S mutation,
Further insights into Pex13p degradation THREE
103
forward primer, used to make
construct pHIPZ12-Pex5- C9S
Pex5-C9S-R GGCGTTGGCAGCAGACTCG
GATCCTCCCAGA
To clone a 596 bp PCR fragment
consisting of the PEX5 promoter
and the 5’ end of PEX5,
introducing the C9S mutation,
reverse primer for first step, used
to make construct
pHIPZ12-Pex5-C9S
Pex5-return CTTTCGGCCTCGTTCATAGC To clone a 754 bp PCR fragment
consisting of the PEX5 promoter
and the PEX5-C9S, reverse
primer for second step, used to
make construct
pHIPZ12-Pex5-C9S
104
4
Chapter 4
Investigating Pex13p degradation in the yeast Saccharomyces cerevisiae
Xin Chen, Srishti Devarajan, Matthias Meurer, Michael Knop and Chris Williams
Author contributions
CW and MK conceived and supervised the project. CW, XC, SD, MM and MK designed
the experiments. XC, SD and CW analysed the data. XC performed biochemical and FM
experiments. SD performed the spot assay, SD and MM performed tFT analysis and data
processing. All authors discussed the results. XC and CW wrote the manuscript, with
contributions from all authors.
FOUR Pex13p degradation in S. cerevisiae
106
Investigating Pex13p degradation in the yeast Saccharomyces cerevisiae
Xin Chen1, Srishti Devarajan
1, Matthias Meurer
2, Michael Knop
2 and Chris Williams
1*
1Cell Biochemistry, Groningen Biomolecular Sciences and Biotechnology Institute,
University of Groningen, 9747AG, the Netherlands 2 Centre for Molecular Biology, University of Heidelberg, Germany
*Corresponding author ([email protected])
Abstract
Pex13p is a member of docking complex required for the import of peroxisomal matrix
proteins. We previously demonstrated that Pex13p is rapidly degraded via the
ubiquitination proteasome system (UPS) in a Pex2p-dependent manner in the yeast
Hansenula polymorpha. However, whether Pex13p degradation is conserved in other
species and which additional factors may be involved remains unclear. In this study, we
demonstrate that UPS-mediated Pex13p degradation occurs in the yeast Saccharomyces
cerevisiae and that the mechanisms of Pex13p degradation are similar to in H.
polymorpha. Additionally, inactivation of Cdc48p, an ATPase involved in degrading
mitochondrial and ER membrane proteins, does not result in stabilization of Pex13p in
vivo, indicating that Pex13p degradation likely occurs via a different mechanism than
other organellar membrane proteins. Furthermore, we utilize a tandem fluorescent
protein timer approach to identify additional factors involved in Pex13p degradation.
Our data demonstrate that cytosolic E2 and E3 enzymes play a role in Pex13p
degradation. Taken together, our data provide further evidence that Pex13p degradation
is conserved throughout evolution while they also uncover novel components of the
UPS that are involved in Pex13p degradation. The implications of our findings are
discussed.
Keywords: Peroxisome/ protein degradation/ Saccharomyces cerevisiae/
ubiquitination/ peroxisomal membrane protein
Pex13p degradation in S. cerevisiae FOUR
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Introduction
Peroxisomes are cellular compartments in eukaryotic cells that house metabolic
pathways. Common functions of peroxisomes include the β-oxidation of fatty acids and
the decomposition of oxygen reactive species, although many species- and cell-specific
peroxisomal functions are known (Gabaldon, 2010). Defects in peroxisome function can
cause a spectrum of inherited developmental brain disorders (Walker et al, 2002).
Peroxisome function depends on which peroxisomal membrane proteins (PMP) and
peroxisomal matrix proteins (MAT) are present in the peroxisome. Both PMPs and
MATs are post-translationally transported to peroxisomes with the aid of receptor
proteins. MATs can be targeted to peroxisomes in one of two different ways: MATs with
a C-terminal peroxisomal targeting signal type-1 (PTS1) sequence can be recognized by
the cytosolic receptor Pex5p, while MATs containing an N-terminal PTS2 signal can be
recognized by Pex7p (Braverman et al, 1997; Mukai et al, 2002). PTS2 protein import
also requires the action of additional co-receptor proteins (Sichting et al, 2003). After
recognition, the receptor-cargo complex binds to the docking complex on the
peroxisomal membrane, consisting of Pex14p and Pex13p (Elgersma et al, 1996;
Johnson et al, 2001). After cargo translocation and release, a process that is poorly
understood (Girzalsky et al, 2010), the receptor Pex5p is ubiquitinated at the peroxisome
by the peroxisomal ubiquitination machinery, consisting of the ubiquitin-conjugating
enzyme Pex4p and the RING finger ubiquitin ligases Pex2p, Pex10p and Pex12p (Platta
et al, 2007; Williams et al, 2008), which allows it to be recycled back to the cytosol,
with the aid of Pex1p and Pex6p, two AAA-ATPases (Platta et al, 2008). The
co-receptor proteins that function with Pex7p in the import of PTS2 proteins can also be
ubiquitinated in similar way during the import cycle (El Magraoui et al, 2013).
Previously, we demonstrated that Hansenula polymorpha Pex13p is degraded via the
ubiquitination proteasome system (UPS), and its degradation requires the peroxisomal
ubiquitination machinery mentioned above (Chen et al, 2018). The UPS-mediated
degradation of proteins occurs in a stepwise fashion (Hershko, 1996). Ubiquitin, a
globular protein of ~8kDa, is first activated by a ubiquitin activating enzyme (E1)
consuming ATP as energy. The activated ubiquitin was then transferred to the Cysteine
residue of a ubiquitin conjugating enzyme (E2). Ubiquitin can then be either passed on
to the active Cysteine of a HECT-class ubiquitin ligase (E3) and subsequently
transferred to a specific substrate, or be transferred to a substrate directly from the E2
with the help of a RING E3 ligase (Scheffner et al, 1995). Attachment of ubiquitin to a
substrate usually occurs via lysine residues on the substrate (Rodriguez, 1996), although
ubiquitin attachment to cysteine, serine and threonine residues has been reported (Wang
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et al, 2007; Williams et al, 2007). In yeast, around 11 E2s and more than 60 E3s are
involved in the ubiquitination process (Finley et al, 2012; Ravid & Hochstrasser, 2007).
While ubiquitination serves many functions, UPS-mediated protein degradation often
requires the attachment of a chain of ubiquitin molecules (referred to as
poly-ubiquitination). Is this case, ubiquitin itself becomes a substrate for ubiquitination
and a common linkage involved in UPS-mediated protein degradation is via Lysine-48
(K48) on ubiquitin (Hershko & Ciechanover, 1998).
In this manuscript, we have investigated the stability of Pex13p in the yeast
Saccharomyces cerevisiae, to establish how conserved the Pex13p degradation process
is across evolution. We demonstrate that Pex13p undergoes rapid degradation in wild
type S. cerevisiae cells and also establish that Pex13p degradation is inhibited when
poly-ubiquitin chain formation is blocked. Furthermore, Pex13p turnover is inhibited in
pex2 and pex4 cells, indicating that the mechanism by which H. polymorpha and S.
cerevisiae Pex13p is degraded is likely to be conserved. Furthermore, we show that the
function of Cdc48p, an AAA-ATPase involved in the degradation of ER and
mitochondrial membrane proteins, is not required for Pex13p degradation. Finally, we
use a high throughput screening approach, combined with a tandem fluorescent timer
(tFT) (Khmelinskii et al, 2014; Khmelinskii et al, 2012), to identify additional proteins
involved in Pex13p degradation. Our tFT and subsequent biochemical analysis identifies
a role for cytosolic E2 and E3 enzymes in Pex13p degradation, providing a solid
platform for future studies aimed at understanding the molecular mechanisms and
underlying functions of Pex13p degradation.
Pex13p degradation in S. cerevisiae FOUR
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Results
The rapid degradation of Pex13p is conserved in S. cerevisiae
Previously we demonstrated that Pex13p in the yeast H. polymorpha undergoes rapid
degradation via the UPS (Chen et al, 2018). In addition, UPS-mediated Pex13p
degradation was reported to occur in plants (Pan et al, 2016), although this degradation
event remain controversial (Ling et al, 2017; Pan & Hu, 2018). Therefore, we decided to
investigate whether Pex13p degradation occurs in other organisms and chose the yeast S.
cerevisiae for this. We utilized Pex13p fused to mGFP, which allowed us to detect the
protein on western blot using anti-GFP antibodies as well as to follow the subcellular
localization of Pex13p using fluorescence microscopy. Cells expressing Pex13-mGFP
are able to grow on media containing oleic acid as sole carbon source (Fig. 1A), a
condition that requires peroxisome function for growth, indicating that Pex13-mGFP is a
functional protein.
To investigate Pex13p turnover, we treated cells expressing Pex13-mGFP with
cycloheximide (CHX). Treatment of cells with CHX blocks protein production and it is
commonly used to investigate the kinetics of protein degradation. Cells were grown on
oleic acid containing media, to stimulate peroxisome proliferation. Pex13-mGFP levels
rapidly decreased after addition of CHX while Pex14p levels remained largely unaltered
(Fig. 1B, D & E), indicating that Pex13-mGFP undergoes protein degradation, similar to
our data in the yeast H. polymorpha (Chen et al, 2018). Next, we investigated the role of
the UPS in Pex13-mGFP degradation. To achieve this, we co-expressed the K48R
mutant form of ubiquitin (Ub) in cells expressing Pex13-mGFP. This Ub-K48R mutant
inhibits the formation of poly-ubiquitination chain on substrates and therefore inhibits
UPS-mediated protein degradation (Thrower et al, 2000). Our data demonstrate that
Pex13-mGFP turnover is significantly reduced in cells expressing Ub-K48R compared
to wild-type (P<0.01), indicating that the UPS is involved in its degradation (Fig. 1C &
D). These data demonstrate that, similar to in H. polymorpha, Pex13p undergoes rapid,
UPS-mediated degradation in S. cerevisiae.
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Fig.1 Rapid degradation of Pex13-mGFP via the UPS occurs in S. cerevisiae.
A Spot assay to test the growth of cells expressing Pex13-tFT or Pex13-mGFP. S.
cerevisiae cells were spotted onto oleic acid plates and cultured at 30℃ for 7 days.
B WT cells expressing Pex13-mGFP were grown on oleic acid containing media for 12 hrs
Pex13p degradation in S. cerevisiae FOUR
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and treated with DMSO (Ctrl) or Cycloheximide (CHX). TCA samples were taken at the
indicated time (hrs) after DMSO/CHX addition and probed by SDS-PAGE and
immunoblotting with antibodies against mGFP, Pex14p and Pyc1p (indicated Pyc).
C Representative western blots of Ub-K48R cells expressing Pex13-mGFP derived from
cells grown and treated as in A. Samples were probed with SDS-PAGE and
immunoblotting with antibodies against mGFP, Pex14p and Pyc1p.
D Quantification of Pex13-mGFP levels in WT and Ub-K48R cells expressing
Pex13-mGFP. Protein levels were normalized to the loading control (Pyc1p) at the
corresponding time point and to the protein levels at T0. Values represent the mean ± SD
of three independent experiments. Asterisks denote statistically significant increases in
protein levels compared to those in WT samples (*P < 0.05, **P < 0.01).
E Quantification of Pex14p levels in WT and Ub-K48R cells expressing Pex13-mGFP.
Protein levels were normalized to the loading control (Pyc1p) at the corresponding time
point and to the protein levels at T0. Values represent the mean ± SD of three
independent experiments.
The peroxisomal ubiquitination machinery is required for Pex13p degradation in S.
cerevisiae
Previously, we demonstrated that Pex13p in the yeast H. polymorpha was stabilized
when components of the peroxisomal ubiquitination machinery, such as the E3 ligase
Pex2p or the E2 Pex4p are absent (Chen et al, 2018). Therefore, we investigated whether
the mechanism by which Pex13p degradation occurs was also conserved in S. cerevisiae.
We introduced Pex13-mGFP into pex2 or pex4 cells and followed Pex13p-mGFP
degradation in CHX-treated cells grown on oleic acid containing media (Fig. 2).
Compared to WT, Pex13-mGFP turnover was clearly inhibited in pex2 (Fig. 2A & B)
and pex4 (Fig. 2 D & E) cells (P<0.001), suggesting that Pex2p and Pex4p play a role in
Pex13p degradation. Next, we investigated the subcellular localization of Pex13-mGFP
in WT and pex2 cells grown on oleic acid containing media. Pex13-mGFP co-localizes
with Pex3-mKate (a stable peroxisomal membrane protein, used as the peroxisomal
membrane marker) on the peroxisomal membrane in pex2 cells (Fig. 3A & B) and
mGFP intensity is significantly increased in pex2 cells (Fig. 3A-D). Furthermore,
Pex13-mGFP levels are significantly elevated in pex2 cells compared to wild-type cells
(Fig. 3E & F), again indicating Pex13-mGFP degradation is inhibited in pex2 cells.
These data strongly suggest that Pex13p degradation in both H. polymorpha and S.
cerevisiae proceeds via a similar mechanism.
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Pex13p degradation in S. cerevisiae FOUR
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Fig.2 Pex13-mGFP degradation is inhibited in cells lacking members of the
peroxisomal ubiquitination machinery
A Representative western blots of pex2 cells expressing Pex13-mGFP derived from cells
grown and treated as in (Fig. 1B). Samples were probed with SDS-PAGE and
immunoblotting with antibodies against mGFP, Pex14p and Pyc1p.
B Quantification of Pex13-mGFP levels in WT and pex2 cells expressing Pex13-mGFP.
Protein levels were normalized to the loading control (Pyc1p) at the corresponding time
point and to the protein levels at T0. Values represent the mean ± SD of three
independent experiments. Values of WT were taken from (Fig. 1A). Asterisks denote
statistically significant increases in protein levels compared to those in WT samples (*P
< 0.05, **P < 0.01, ***P < 0.001).
C Quantification of Pex14p levels in WT and pex2 cells. Protein levels were normalized to
the loading control (Pyc1p) at the corresponding time point and to the protein levels at
T0. Values represent the mean ± SD of three independent experiments. Values of WT
were taken from Fig. 1B.
D Representative western blots of pex4 cells expressing Pex13-mGFP derived from cells
grown and treated as in (A). Samples were probed with SDS-PAGE and immunoblotting
with antibodies against mGFP, Pex14p and Pyc1p.
E Quantification of Pex13-mGFP levels in WT and pex4 cells expressing Pex13-mGFP.
Protein levels were normalized to the loading control (Pyc1p) at the corresponding time
point and to the protein levels at T0. Values represent the mean ± SD of three
independent experiments. Values of WT were same as in (Fig. 1B). Asterisks denote
statistically significant increases in protein levels compared to those in WT samples (*P
< 0.05, **P < 0.01, ***P < 0.001).
F Quantification of Pex14p levels in WT and pex4 cells. Protein levels were normalized to
the loading control (Pyc1p) at the corresponding time point and to the protein levels at
T0. Values represent the mean ± SD of three independent experiments. Values of WT
were same as in (Fig. 1B).
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Fig.3 Pex13-mGFP accumulates on peroxisomes in pex2 cells.
A WT and pex2 cells producing Pex13-mGFP and Pex3-mKate2 were grown on oleic acid
containing media to an OD600 of 1.0 and fluorescence microscopy images were taken.
Images of Pex13-mGFP were processed using ImageJ with optimal settings to show
signals in WT and pex2. Pex3-mKate2 was used as peroxisomal membrane marker. The
following settings were used: for WT cells mGFP (290, 650) and mKate2 (225, 600); for
pex2 cells mGFP (290, 2900) and mKate2 (225, 630). Scale bar: 5μm.
B Fluorescence images of Pex13-mGFP in WT or pex2 shown in (A) were processed using
Pex13p degradation in S. cerevisiae FOUR
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ImageJ with the same settings: mGFP (300, 2000), mKate2 (225, 620). Scale bar: 5μm.
C Box plot showing quantification of mGFP fluorescence intensity at the peroxisomal
membrane in WT and pex2 cells producing Pex13-mGFP. Fluorescence intensities
(arbitrary units) were measured using ImageJ. The box represents values from the 25
percentile to the 75 percentile; the horizontal line through the box represents the median
value. Whiskers indicate maximum and minimum values. Pex13-mGFP measurements
were taken as described in the Materials and Methods section.
D Average ratio ± SD per cell (n = 40) of mGFP to mKate intensities in WT and pex2 cells.
***P < 0.001.
E WT and pex2 cells producing Pex13-mGFP grown on oleic acid media and TCA samples
were taken when the cultures reached an OD600 of 1.0. Samples were subjected to
SDS-PAGE and immunoblotting using antibodies against mGFP, Pex14p and Pyc1p.
F Quantification of protein levels in WT and pex2 cells, normalized to the loading control
Pyc1p. Protein levels in WT cells were set to 1. Values represent the mean ± SD of three
independent experiments. Asterisks denote statistically significant increases in protein
levels compared to those in WT samples (**P < 0.01).
Cdc48p function is not required for Pex13p degradation
Membrane proteins need to be removed from their native membrane environment before
they can be degraded by the proteasome and the AAA-ATPase Cdc48p (p97 in humans)
is known to extract membrane proteins from both the endoplasmic reticulum (ER) and
mitochondrial membranes and deliver them to the proteasome for degradation (Cao et al,
2003; Wolf & Stolz, 2012). Therefore, we considered the possibility that Cdc48p could
be involved in extracting Pex13p out of the peroxisomal membrane and delivering it to
the proteasome, for degradation. To investigate this, we utilized a temperature sensitive
mutant form of Cdc48p (cdc48-3), since CDC48 is an essential gene (Dargemont &
Ossareh-Nazari, 2012; Wolf & Stolz, 2012; Yamanaka et al, 2012). The mutant Cdc48
protein is active when cells are grown at the permissive temperature of 23℃ but is
inactive when cells are grown at the restrictive temperature of 37℃. We used Cdc5p as a
control substrate. Cdc5p is a serine/threonine-protein kinase required for the cell cycle
and its degradation requires Cdc48p (Cao et al, 2003). We introduced Pex13-mGFP or
Cdc5-HA6 into cdc48-3 cells and followed the degradation of these proteins in oleic
acid-grown cells treated with CHX, at both 23℃ and 37℃ (Fig. 4). Cdc5-HA6
degradation was observed in cells grown at the permissive temperature while Cdc5-HA6
turnover was inhibited in cells growing at the restrictive temperature (Fig. 4A-C).
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Significantly, Pex13-mGFP was degraded at a similar rate in cells grown at both the
permissive and the restrictive temperatures (Fig. 4D-K), suggesting that Cdc48p
function is not required for Pex13p degradation.
(main text continued in p.119)
Fig.4 Cdc48p function is not required for Pex13p degradation.
A Representative western blots of cdc48-3 cells expressing Cdc5-HA6 derived from cells
grown and treated as in (A). Samples were probed with SDS-PAGE and immunoblotting
with antibodies against HA and Pyc1p.
B Representative western blots of cdc48-3 cells expressing Cdc5-HA6 derived from cells
grown and treated as in (E). Samples were probed with SDS-PAGE and immunoblotting
with antibodies against HA and Pyc1p.
C Quantification of Cdc5-HA6 levels in cdc48-3 cells at permissive temperature 23℃ or
restrictive temperature 37℃ expressing. Protein levels were normalized to the loading
control (Pyc1p) at the corresponding time point and to the protein levels at T0. Values
represent the mean ± SD of three independent experiments. (*P < 0.05)
D WT cells expressing Pex13-mGFP were grown on oleic acid media at 23℃ for 18 hrs and
treated with DMSO (Ctrl) or Cycloheximide (CHX). TCA samples were taken at the
indicated time (hrs) after DMSO/CHX addition and probed by SDS-PAGE and
immunoblotting with antibodies against mGFP, Pex14p and Pyc1p.
(Fig. 4D, continued in next page)
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(Fig.4D, continued from previous page)
E Representative western blots of cdc48-3 cells expressing Pex13-mGFP derived from
cells grown and treated as in (A). Samples were probed with SDS-PAGE and
immunoblotting with antibodies against mGFP, Pex14p and Pyc1p.
F Quantification of Pex13-mGFP in (A) and (B). Protein levels were normalized to the
loading control (Pyc1p) at the corresponding time point and to the protein levels at T0.
Values represent the mean ± SD of three independent experiments.
G Quantification of Pex14p levels in WT and cdc48-3 cells expressing Pex13-mGFP.
Protein levels were normalized to the loading control (Pyc1p) at the corresponding time
point and to the protein levels at T0. Values represent the mean ± SD of three
independent experiments.
(Fig. 4H, continued in next page)
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(Fig.4D, continued from previous page)
H WT cells expressing Pex13-mGFP were grown on oleic acid media at 23℃ for 17 hrs,
then shifted to 37℃ for 1 hr, and treated with DMSO (Ctrl) or Cycloheximide (CHX).
TCA samples were taken at the indicated time (hrs) after DMSO/CHX addition and
probed by SDS-PAGE and immunoblotting with antibodies against mGFP, Pex14p and
Pyc1p.
I Representative western blots of WT cells expressing Pex13-mGFP derived from cells
grown and treated as in (E). Samples were probed with SDS-PAGE and immunoblotting
with antibodies against mGFP, Pex14p and Pyc1p.
J Quantification of Pex13-mGFP in (E) and (F). Protein levels were normalized to the
loading control (Pyc1p) at the corresponding time point and to the protein levels at T0.
Values represent the mean ± SD of three independent experiments.
K Quantification of Pex14p levels in WT and cdc48-3 cells expressing Pex13-mGFP.
Protein levels were normalized to the loading control (Pyc1p) at the corresponding time
point and to the protein levels at T0. Values represent the mean ± SD of three
independent experiments.
Pex13p degradation in S. cerevisiae FOUR
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Investigating Pex13p degradation with a tandem fluorescent timer
While our data demonstrate a role for the peroxisomal ubiquitination machinery in the
degradation of S. cerevisiae Pex13p (Fig. 2 and 3), we sought to identify which
additional factors may regulate Pex13p degradation. To achieve this we utilized a
tandem fluorescent timer (tFT) approach, which has been previously used to study
protein stability in S. cerevisiae cells (Khmelinskii et al, 2014). The tFT tag consists of
mCherry and sfGFP, which have maturation half times of around 45 and 5 minutes,
respectively (in S. cerevisiae cells grown at 30°C). Measuring the red and green
fluorescent intensities directly in cells can provide information on the relative stability
of the tFT-tagged protein in an in vivo setting. A high mCherry/sfGFP intensity ratio
indicates that the tagged protein is stable while a low mCherry/sfGFP ratio indicates an
unstable protein (Khmelinskii et al, 2012). Cells expressing Pex13-tFT only (and hence
not the WT version of the protein) can grow on oleic acid (Fig. 1A), suggesting that the
Pex13-tFT protein is functional. Furthermore, Pex13-tFT was rapidly degraded in cells
treated with CHX (Fig. 5), demonstrating that Pex13-tFT can be used to study Pex13p
degradation.
Figure 5. Pex13-tFT is rapidly degraded in S. cerevisiae cells treated with CHX.
A Representative western blots of samples derived from cells expressing Pex13-tFT or
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Pex11-tFT grown for 12 hrs on oleic acid media. Blots were probed with antibodies
directed against mGFP and Pyc1p. * Denotes a hydrolysed product of mature mCherry
during SDS-sample preparation due to chemical breakage of the fluorophore. This cuts
mCherry into two pieces, at around position 69 of mCherry, thereby generating a
fragment containing the C-term mCherry and sfGFP of approximately 45 kDa. #
Denotes an incomplete degradation product of sfGFP due to its rigid fold. This 33 kDa
band often appears as a doublet. The presence of this band is a strong signature that the
tFT tagged protein is degraded by the proteasome (Khmelinskii et al, 2016).
B Quantification of Pex13-tFT and Pex11-tFT levels of blots in the left. Protein levels
were normalized to the loading control (Pyc1p) at the corresponding time point and to
the protein levels at T0. Values represent the mean ± SD of three independent
experiments.
Next, we created a library of 152 strains made by synthetic genetic array (SGA)
expressing Pex13-tFT that either lacked a gene involved in protein degradation or which
contained a mutant version of a protein involved in protein degradation (in case the
deletion was lethal) (Tong & Boone, 2006). Gene deletion and gene tagging were
validated by PCR (data not shown). Mutant cells expressing Pex13-tFT were grown on
synthetic complete media plates containing 0.1% oleic acid and 0.1% glucose for seven
days at 30°C. Colonies (four technical replicates for each mutant strain plus controls)
were imaged every day to determine mCherry and GFP fluorescence intensities and the
average ratio of mCherry to sfGFP intensities was determined for each strain on each
day. These ratios were normalized to the ratio measured in WT cells expressing
Pex13-tFT and the Z-score, the deviation of the ratio for a particular mutant strain
compared to the average ratio across all strains, was calculated for each strain (Fig. 6).
Further details on how the images were taken and the data were processed can be found
in the Materials and Methods section.
We considered mutant strains that displayed an increase in Z-score of more than 1.0
on each of the seven days potentially interesting. These strains, which include cells
deleted for PEX4, PEX2, PEX10, PEX12 and UBI4 (which depletes the amount of
ubiquitin available in the cell, but does not result in an absence of ubiquitin completely
because of the presence of additional copies of the UBI gene), display an increase in
Pex13-tFT stability on each of the seven days (Fig. 6). A role for these factors in Pex13p
degradation was already shown (Fig. 1, 2 & 3), validating our tFT approach. In addition,
cells deleted for UBR2, UFD4, RCY1, YUH1, UBP6 and UBC4 all displayed increased
Pex13p degradation in S. cerevisiae FOUR
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Pex13-tFT stability on each of the seven days (Fig. 6). Ufd4p is a cytosolic HECT E3
ligase which regulates the degradation of misfolded proteins (Theodoraki et al, 2012).
Interestingly, Ufd4p is also involved in the degradation of Pxa1p (Devarajan et al, in
preparation), a peroxisomal membrane protein involved in the import of activated
long-chain fatty acids from the cytosol to the peroxisomal matrix (Shani et al, 1995).
Ubc4p is a ubiquitin-conjugating enzyme (E2) involved in the degradation of abnormal
or excess proteins while it also mediates the ubiquitination of Pex5p (Seufert & Jentsch,
1990; Williams et al, 2007). Ubc4p is known to work with Ufd4p in the ubiquitination
of certain substrates (Bao, 2015). Ubr2p is a cytosolic RING E3 ligase which like Ufd4p,
is involved in the degradation of misfolded proteins (Nillegoda et al, 2010). S. cerevisiae
cells depleted of Ubr2p cannot grow on oleic acid containing media (Lockshon et al,
2007; Saleem et al, 2010), although the underlying peroxisomal defect in these cells is
unknown. Ubp6p is a de-ubiquitinating enzyme that associates with the proteasome and
can negatively regulate proteasomal activity (Hanna et al, 2006) and it is also involved
in Pxa1p degradation (Devarajan et al, in preparation). Rcy1p is involved in recycling
plasma membrane proteins internalized by endocytosis (Wiederkehr et al, 2000) and is
required for recycling of the v-SNARE Snc1p (Galan et al, 2001). Yuh1p is a
de-ubiquitinating enzyme that regulates cellular ubiquitin levels (Miller et al, 1989).
Taken together, our tFT analysis identifies additional factors potentially involved in
Pex13p degradation.
Ufd4p, Ubc4p and Ubr2p facilitate the targeted degradation of Pex13p
Our tFT data identified six additional candidates that could play a role in Pex13p
degradation and we chose to investigate the role of three of these candidates in Pex13p
turnover. These were the cytosolic E2 Ubc4p and the cytosolic E3 ligases Ufd4p and
Ubr2p. As negative control we chose atg12 cells, since no increase in Pex13-tFT
stability was observed in these cells (Fig. 6). We introduced Pex13-mGFP into ufd4,
ubc4, ubr2 and atg12 cells and investigated Pex13-mGFP steady state levels in cells
grown on oleic acid containing media, establishing that Pex13-mGFP levels are
significantly elevated ufd4, ubr2 and ubc4 cells (Fig. 7). In addition, degradation of
Pex13-mGFP proceeded at a significantly lower rate in CHX treated ufd4 (Fig. 8), ubc4
(Fig. 9) and ubr2 (Fig. 10) cells, supporting our data on the steady state levels of
Pex13-mGFP in these mutant strains (Fig. 7A,B). Taken together, these data provide
further evidence for a role for Ufd4p, Ubc4p and Ubr2p in Pex13-mGFP degradation.
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Fig.6 tFT analysis identifies additional factors involved in Pex13p degradation.
Heat-map indicating relative Pex13-tFT stability in different mutant yeast strains. Strains
expressing Pex13-tFT were grown for seven days at 30℃ on oleic acid plates with 0.1%
glucose (w/v). The mCherry and sfGFP fluorescence intensities were measured for colonies
from each strain on each day and the mCherry/sfGFP ratio was calculated and used to
determine the Z-score, the deviation of the ratio for a particular strain on a particular day
compared to the average ratio across all strains on that day. Increases in Z-score are colour
coded, ranging from 1.0 or less (green) to 5.0 (red). The data for each square in the heat map
are derived from four technical replicates.
Fig.7 Pex13-mGFP levels are increased in ufd4, ubr2 and ubc4 cells.
A Representative western blots of samples derived from WT and mutant cells grown for 12
hrs on oleic acid media. The atg12 strain was used as a negative control. Blots were
probed with antibodies directed against mGFP, Pex14p and Pyc1p.
B Quantification of protein levels in WT and mutant cells, normalized to the loading
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control Pyc1p. Protein levels in WT cells were set to 1. Values represent the mean ± SD
of three independent experiments. Asterisks denote statistically significant increases in
protein levels compared to those in WT samples (*P < 0.05, **P < 0.01).
Fig.8 Cells lacking the cytosolic E3 Ufd4p display enhanced Pex13-mGFP stability.
A The ufd4 cells expressing Pex13-mGFP were grown on oleic acid media for 12 hrs and
treated with DMSO (Ctrl) or Cycloheximide (CHX). TCA samples were taken at the
indicated time (hrs) after DMSO/CHX addition and probed by SDS-PAGE and
immunoblotting with antibodies against mGFP, Pex14p and Pyc1p.
B Quantification of Pex13-mGFP level in ufd4 cells expressing Pex13-mGFP. Protein
Pex13p degradation in S. cerevisiae FOUR
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levels were normalized to the loading control (Pyc1p) at the corresponding time point
and to the protein levels at T0. Values represent the mean ± SD of three independent
experiments. Values of WT were same as in (Fig. 1B). Asterisks denote statistically
significant increases in protein levels compared to those in WT samples (*P < 0.05).
C Quantification of Pex14p level in ufd4 cells expressing Pex13-mGFP. Protein levels
were normalized to the loading control (Pyc1p) at the corresponding time point and to
the protein levels at T0. Values represent the mean ± SD of three independent
experiments. Values of WT were same as in (Fig. 1B).
Fig.9 The cytosolic E2 Ubc4 is involved in Pex13-mGFP degradation.
A The ubc4 cells expressing Pex13-mGFP were grown on oleic acid media for 12 hrs and
FOUR Pex13p degradation in S. cerevisiae
126
treated with DMSO (Ctrl) or Cycloheximide (CHX). TCA samples were taken at the
indicated time (hrs) after DMSO/CHX addition and probed by SDS-PAGE and
immunoblotting with antibodies against mGFP, Pex14p and Pyc1p.
(Fig. 9B, continued in next page)
Fig.10 Deletion of UBR2, which encodes for a cytosolic RING E3 ligase, impacts on
Pex13-mGFP degradation.
A The ubr2 cells expressing Pex13-mGFP were grown on oleic acid media for 12 hrs and
treated with DMSO (Ctrl) or Cycloheximide (CHX). TCA samples were taken at the
indicated time (hrs) after DMSO/CHX addition and probed by SDS-PAGE and
Pex13p degradation in S. cerevisiae FOUR
127
immunoblotting with antibodies against mGFP, Pex14p and Pyc1p.
B Quantification of Pex13-mGFP levels in WT and ubr2 cells expressing Pex13-mGFP.
Protein levels were normalized to the loading control (Pyc1p) at the corresponding time
point and to the protein levels at T0. Values represent the mean ± SD of three
independent experiments. Values of WT were same as in (Fig. 1B). Asterisks denote
statistically significant increases in protein levels compared to those in WT samples (*P
< 0.05, **P < 0.01).
C Quantification of Pex14p levels in WT and ubr2 cells expressing Pex13-mGFP. Protein
levels were normalized to the loading control (Pyc1p) at the corresponding time point
and to the protein levels at T0. Values represent the mean ± SD of three independent
experiments. Values of WT were same as in (Fig. 1B).
__________________
(Fig. 9B, continued from previous page)
B Quantification of Pex13-mGFP level in ubc4 cells expressing Pex13-mGFP. Protein
levels were normalized to the loading control (Pyc1p) at the corresponding time point
and to the protein levels at T0. Values represent the mean ± SD of three independent
experiments. Values of WT were same as in (Fig. 1B). Asterisks denote statistically
significant increases in protein levels compared to those in WT samples (*P < 0.05).
C Quantification of Pex14p level in ubc4 cells expressing Pex13-mGFP. Protein levels
were normalized to the loading control (Pyc1p) at the corresponding time point and to
the protein levels at T0. Values represent the mean ± SD of three independent
experiments. Values of WT were same as in (Fig. 1B).
Discussion
Pex13p is a PMP and member of the peroxisomal docking complex which is required for
MAT import, although its actual role in the import process is still unclear. Pex13p has a
relatively short half-life in the yeast H. polymorpha and it is degraded via the UPS in a
Pex2p-dependent manner (Chen et al, 2018) In addition Arabidopsis Pex13p can be
degraded by the UPS, in a process involving the RING E3 Ligase SP1 (Pan et al, 2016).
Together, these reports suggest that UPS-mediated Pex13p degradation is a conserved
process, which led us to investigate Pex13p degradation in the yeast S. cerevisiae. Our
data clearly establish that Pex13p is degraded in S. cerevisiae while additionally
demonstrating that Pex13p degradation likely proceeds via a similar UPS-mediated
mechanism to that in H. polymorpha. Although the function of Pex13p degradation
remains unclear (see Chapter 3 of this thesis), the fact that it has been shown to occur in
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three different organisms strongly suggests that Pex13p degradation is fundamental to
peroxisomes. This poses the question as to whether Pex13p degradation also occurs in
humans and if so, what would be the impact of blocking Pex13p degradation on human
health? Mutations in Pex2p, Pex10p or Pex12p have been reported in patients suffering
from peroxisome biogenesis disorders (Gootjes et al, 2004a; Gootjes et al, 2004b;
Warren et al, 2000). In many cases the RING E3 complex members displayed reduced
activity or loss of function, which resulted in defects in peroxisomal MAT import
(Krause et al, 2006). It is probable that many of the defects exhibited by these patients
are caused by inhibitions to Pex5p recycling. Nevertheless, because the peroxisomal E3
ligases are clearly involved in Pex13p degradation, it is feasible that some of the effects
displayed by patients with reduced peroxisomal E3 ligase activity may stem from
blocking Pex13p degradation.
Cdc48p is an AAA-ATPase involved in protein degradation and it is able to extract
ubiquitinated substrates from the ER and mitochondrial membranes and target them to
the proteasome for degradation (Wolf & Stolz, 2012). However, since our data establish
that Cdc48p function is not required for Pex13p degradation, it remains unknown how
ubiquitinated Pex13p may target to the proteasome. One possibility is that another
AAA-ATPase regulates the transport of Pex13p towards the proteasome. Pex1p and
Pex6p are two such ATPases that form a complex and can extract ubiquitinated Pex5p
from the peroxisomal membrane (Platta et al, 2008), although Pex3p degradation in H.
polymorpha did not require Pex1p (Williams & van der Klei, 2013b). This may argue
against a role for the Pex1p/Pex6p complex in Pex13p degradation. Similarly the
membrane bound AAA-ATPase Msp1p, which was reported to extract tail anchored
proteins out of the peroxisomal membrane for degradation (Weir et al, 2017), is also a
potential candidate to fulfil this function. Another possibility is that the cytosolic
proteasome approaches ubiquitinated Pex13p while still at the peroxisomal membrane.
The proteasome can associate with the ER membrane (Lipson et al, 2008; Mayer et al,
1998), which led Mayer et al. to propose that dislocation and degradation are coupled
(Mayer et al, 1998). They further proposed that Cdc48p and Rpt4p (a subunit of 19S
regulatory particle of the proteasome) might work in parallel, due to their structural
(both are hexameric AAA-ATPases) and functional (both can bind ubiquitin conjugates)
similarities (Dai & Li, 2001; Elsasser & Finley, 2005; Lam et al, 2002). In such a model,
the proteasome may not require the action of an additional AAA-ATPase to facilitate
Pex13p degradation. Clearly further work is needed to investigate how ubiquitinated
Pex13p is extracted from the peroxisomal membrane.
Using a tandem fluorescent timer (tFT) and high throughput screening approach,
Pex13p degradation in S. cerevisiae FOUR
129
we observed that, in addition to in cells lacking members of the peroxisomal
ubiquitination machinery, Pex13-tFT stability was also increased in cells lacking Ufd4p,
Ubc4p or Ubr2p. Furthermore the steady state levels of Pex13-mGFP was increased
while Pex13-mGFP degradation was reduced in each of these deletion strains. Together
these data strongly suggest that Ufd4p, Ubr2p and Ubc4p play a role in Pex13-mGFP
degradation. This raises the question what is the relationship between the different E2s
and E3s that play a role in Pex13p degradation? One possibility is that several pathways
act in parallel on Pex13p. One pathway may rely on the peroxisomal ubiquitination
machinery while another may require Ubc4p as E2 and Ufd4p or Ubr2p as E3. Ubc4p is
known to act as E2 for Ufd4p (Bao, 2015). However, another option is that all these
factors act together in ubiquitinating Pex13p. Ufd4p can associate with the RING E3
ligase Ubr1p, which allows the rapid formation of poly-ubiquitin chains on substrates
(Hwang et al, 2010). Perhaps this is also the case for Pex13p, with Ufd4p, Ubr2p and
Ubc4p “joining forces” with Pex4p and the peroxisomal E3 ligases to promote the rapid
formation of poly-ubiquitinated Pex13p, to facilitate its degradation. Nevertheless,
deletion of PEX2 or PEX4 has a dramatic effect on Pex13-mGFP degradation (Fig. 2)
whereas deletion of UFD4, UBR2 or UBC4 has a smaller impact on Pex13-mGFP
degradation (Fig. 7-10). These data could suggest that the peroxisomal ubiquitination
machinery is the major player in Pex13p degradation, while the cytosolic factors Ufd4p,
Ubc4p and Ubr2p play a more minor role (Fig. 11). However, further investigations are
required, including the potential roles of the other factors identified in our tFT analysis
in Pex13p degradation.
In summary, our results demonstrate that Pex13p degradation is a general process
conserved across different organisms yet occurring likely via similar mechanisms while
they also identify roles for additional, cytosolic E2s and E3s in Pex13p degradation.
However, further study is required before the mechanisms that underlie Pex13p
degradation become clear.
FOUR Pex13p degradation in S. cerevisiae
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Fig.11 A schematic model of Pex13p degradation.
The ubiquitination machinery at the peroxisomal membrane, including Pex4p (E2) and
RING complex Pex2p/ Pex10p/ Pex12p (E3), plays a major role in Pex13p ubiquitination.
The cytosolic factors Ufd4p, Ubc4p and Ubr2p play a more minor role, possibly involved in
a later step of poly-ubiquitination chain formation.
Pex13p degradation in S. cerevisiae FOUR
131
Materials and Methods
Molecular techniques and construction of S. cerevisiae strains
S. cerevisiae strains used in this study are listed in Table 1. Strains used in tFT analysis
were constructed as described previously (Khmelinskii et al, 2014). The plasmids and
primers used in this study are listed in Table 2 and 3 respectively. Phusion DNA
polymerase (Thermo Scientific) was used to produce gene fragments.
Competent cells of S. cerevisiae were prepared as follows: Cells were inoculated in
20 mL YPD liquid media and incubated with shaking of 200 rpm overnight at 30℃. The
OD 600 of the overnight culture was measured and cells were diluted to 0.25 in 50 mL
YPD. The cells were harvested at 5000 rpm for 5 min when the OD 600 reached 0.8~
1.0. Cells were washed twice with sterile water, once with 5 mL of 1 M Sorbitol, and
suspended in 300 μL of 1 M Sorbitol. The competent cells were aliquoted into 50 μL and
frozen at -80℃.
For S. cerevisiae transformation, 15 μL of PCR product, 40 μL of denatured salmon
sperm DNA (100℃ for 10 min, and immediately cooled on ice-water) and 300 μL of
PEG/ LiAc/ TE solution (0.8 mL 50% PEG-3350, 0.1 mL 100 mM Tris-HCl pH7.5 with
10 mM EDTA, 0.1 mL 1M Lithium acetate) were mixed with 50 μL of cells and shaken
for 30 min at 30℃. Cells were mixed with 40 μL DMSO and heat shocked for 15 min at
42℃. Cells were cooled on ice for 1 min and washed once with 1mL YPD. Cells were
finally resuspended in 5 mL YPD, shaken for 2~ 3 hr at 30℃ and plated on either YPD
plates containing appropriate antibiotics or, for cells expressing Ub-K48R, on YND
plates without Uracil. Plates were grown at 30℃ for 2 to 3 days.
The Pex13-mGFP fragment was prepared as follows: The plasmid
pHIPZ-Pex13-mGFP containing H. polymorpha Pex13-mGFP and Zeocin resistance
gene was used as the template. The Zeocin fragment together with its promoter and
terminator was obtained by PCR using the primers ScPex13-mGFP-F and
Tcyc1-dnScP13-R, resulting in a product of 2240 bp with homologous region of
upstream and downstream to PEX13 at both ends. This PCR-based fragment was used
for transformation to obtain strains expressing Pex13-mGFP.
To produce the Pex3-mKate fragment, the plasmid pHIPH-Pex14-mKate2
containing H. polymorpha Pex14-mKate2 and Hygromycin resistance gene was used as
template. The Hygromycin fragment, together with its promoter and terminator, was
obtained by PCR using the primers ScPex3-mKate-F_SRI and ScPex3-mKate-R_SRI,
resulting in a product of 2858 bp with homologous region of upstream and downstream
to PEX3. This fragment was transformed into yeast, to obtains strains expressing
Pex3-mKate.
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The Cdc5-HA6 fragment was prepared as follows: A HA6 fragment and
Hygromycin cassette, together with its promoter and terminator sequences, was obtained
by PCR using the primers ScCdc5-HA6-F and HYG-dnCdc5-R and the plasmid
pHIPH-AID-HA6 as template. The resulting 1724 bp product, containing sequences
homologous to the upstream and downstream regions of S. cerevisiae CDC5, was used
for transformation, to obtain a cdc48-3 strain expressing Cdc5-HA6.
The episomal plasmid Yep-Pcup1-myc-Ub-K48R has myc-Ub-K48R cassette under
control of Copper promoter (Pcup1-overexpression promoter), with URA3 marker for
selection in yeast. Yeast episomal plasmids, unlike genome integration, are high copy
plasmids and remain free in the cell. PCR of CUP1 promoter was performed on the
plasmid pCGCN-FAA4-mGFP using primers NotI-CUP1-F and CUP1-BamHI-R,
resulting a fragment of 347 bp. The fragment was further digested with NotI and BamHI,
and cloned into NotI/ BamHI digested pRDV2 vector, generating
pHIPH-Pcup1-myc-Ub-K48R. PCR was performed on the plasmid
pHIPH-Pcup1-myc-Ub-K48R with primers NotI-CUP1-F and UbKR-SacI-R, resulting a
632 bp fragment which was digested with NotI and SacI and cloned into NotI/ SacI
digested pRG226 (ADDGENE), producing a plasmid of 5979 bp, termed as
Yep-Pcup1-myc-Ub-K48R.
PEX11 and PEX13 were endogenously and seamlessly tagged by PCR targeting
with tFT as previously described (Khmelinskii et al, 2014; Khmelinskii et al, 2011).
All integrations were confirmed by colony PCR using Phire Hot Start II (Thermo
Scientific). Strains containing Pex13-mGFP were further checked by fluorescence
microscopy and Western blotting and strains containing Pex3-mKate were further
checked by fluorescence microscopy.
Strains and growth conditions
Yeast transformants were selected on YPD plates containing 2% agar and 100 μg/ml
Zeocin (Invitrogen) or 300 μg/ml Hygromycin (Invitrogen) or on YND plates (6.7g/L
Yeast Nitrogen base w/o Amino acids (DIFCO), 5g/L Glucose (BOOM B.V.)) containing
2% agar, for the Ub-K48R strain. The E. coli strain DH5α was used for cloning
purposes. E. coli cells were grown in LB supplemented with 100 μg/ml Ampicillin at
37 °C. For selection of auxotrophic transformants, selective minimal medium was
supplemented with 2% glucose and the required amino acids mixture. Cycloheximide
(CHX) when used, was added to a final concentration of 6 mg/ml.
All S. cerevisiae liquid cultures were gown while shaking at 200 rpm. S. cerevisiae
cells for TCA lysates, CHX assays and fluorescence microscopy were grown on YM2
Pex13p degradation in S. cerevisiae FOUR
133
media (6.7g/L Yeast Nitrogen base w/o Amino acids (DIFCO), 10g/L Casein hydrolysate
(Sigma), 0.06g/L Uracil (Sigma) and 0.06g/L L-Tryptophan (Sigma)). Cells were first
grown on YM2 supplemented with 2% glucose at 30℃ overnight, then transfer to YM2
plus 0.3% glucose at 2pm on day-2 and grown at 30℃ for 8 hr. Finally cells were
transferred to YM2 plus 0.1% oleic acid (Sigma), 0.1% glucose and 0.05% Tween-80
(YM2O) and grown at 30℃ till an OD600 of around 1.0 (~10-12hr), after which cells
were either harvested for TCA lysates or CHX/fluorescence microscopy experiments
were performed.
For experiments using the Cdc48 temperature sensitive strain cdc48-3, cells
expressing Pex13-mGFP were grown on YM2 plus 2% glucose at 23℃ overnight, then
at 10am on day-2 cells were transferred to YM2 plus 0.3% glucose and grown at 23℃
for 12hr. Finally, cells were transferred to YM2O media and grown further at 23℃. After
17hrs of growth, cells were split into two groups, those for CHX treatment at the
permissive (23℃) temperature and those for CHX treatment at the restrictive (37℃)
temperature. For permissive-temperature growth, cells were grown on YM2O media for
a further 1hr at 23℃ and treated with DMSO or CHX. For restrictive temperature growth,
cells were shifted to 37℃ for 1 hr, treated with DMSO or CHX and grown further at 37℃.
Preparation of yeasts TCA lysates
Cell extracts of TCA-treated cells were prepared for SDS-PAGE as detailed previously
(Baerends et al, 2000). Three OD600 units of cells from each culture (at each time point)
were taken for TCA lysis so that the amount of cells is constant, and after TCA lysis,
equal volume (10μL) of each sample was loaded per lane and blots were probed with
rabbit polyclonal antisera raised against the Myc tag (Santa Cruz Biotech, sc-789),
Pex14p (Bottger et al, 2000), or pyruvate carboxylase 1 (Pyc1p) (Fahimi et al, 1993) or
mouse monoclonal antisera raised against HA tag (Sigma, H3663) or mGFP (Santa Cruz
Biotech, sc-9996). Secondary goat anti-rabbit (31460) or goat anti-mouse (31430)
antibodies conjugated to horseradish peroxidase (Thermo Fisher Scientific) were used
for detection. Pyc1p was used as a loading control.
Quantification of Western blots
Blots were scanned by using a densitometer (GS-710; Bio-Rad Laboratories) and
protein levels were quantified using Image Studio Lite Ver5.2 software (LI-COR
Biosciences). In the case of Pex14p blots, both the phosphorylated and
unphosphorylated forms were included in the calculation if both forms were visible. The
value obtained for each band was normalized by dividing it by the value of the
FOUR Pex13p degradation in S. cerevisiae
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corresponding Pyc1p band (loading control). For comparison of absolute protein levels
(Figures 2 and 4), normalized values obtained for Pex13p and Pex14p levels in WT cells
were set to 1 and the levels of these proteins in mutant cells are displayed relative to WT.
For CHX experiments (Figures 1, 5, 6 and 7), the normalized values of T0 samples were
set to 1.0 and values obtained from the T1-T3 samples are displayed as a fraction of T0
values. Standard deviations were calculated using Excel. * represents P-values < 0.05,
** represents P-values < 0.01 and *** represents P-values < 0.001. The data presented
are derived from three independent experiments.
Fluorescence Microscopy
All fluorescence microscopy images were acquired using a 100×1.30 NA Plan-Neofluar
objective (Carl Zeiss). Wide-field microscopy images were captured by an inverted
microscope (Axio Scope A1, Carl Zeiss) using Micro-Manager software and a digital
camera (CoolSNAP HQ2; Photometrics). GFP signal was visualized with a 470/440-nm
band pass excitation filter, a 495-nm dichromatic mirror, and a 525/550-nm band pass
emission filter. mKate signal was visualized with a 587/525-nm band pass excitation
filter, a 605-nm dichromatic mirror, and a 647/670-nm band-pass emission filter.
For images taken of Pex13-mGFP in WT grown on oleic acid containing medium,
the optimal settings were mGFP (290, 650) and mKate2 (225, 600), and in pex2, the
optimal settings mGFP (290, 2900) and mKate2 (225, 630) were applied for processing.
The general settings used to compare the signal of Pex13-mGFP in WT and pex2, mGFP
(300, 2000) and mKate2 (225, 620) were applied for processing.
For quantification of the Pex13-mGFP signal in WT or pex2 cells, a rectangular
area was drawn using the “rectangular tool” from ImageJ (Abramoff et al, 2004) to
envelope the region containing the Pex13-mGFP spot and pixel intensity inside the area
was measured. The measured maximum fluorescence intensity of GFP on peroxisomes
was corrected for the background intensity and a box plot was made using Microsoft
Excel. The box represents values from the 25 percentile to the 75 percentile; the
horizontal line through the box represents the median value. Whiskers indicate
maximum and minimum values.
Spot assay
The yeast cells were grown while shaking overnight at 30 °C on YM2 medium
containing 2% glucose. Cells were harvested and washed with water. Each strain with
cells diluted to an OD600nm of 0.1 for the first dilution. The following dilutions were
made successively with 10 μL of previous dilution liquid and 90 μL water. Then 5 μL of
Pex13p degradation in S. cerevisiae FOUR
135
ten-fold serial dilutions of each yeast culture was spotted onto oleic acid plates (YM2O).
The gradient dilution concentrations are specified in figure legends. Growth difference
was measured after incubation at 30 °C for 48 h.
Tandem fluorescent timer (tFT) analysis
The tFT analysis in this study is mainly based on previous established tFT technique,
and the following procedure is adapted from the detailed protocols already published
(Khmelinskii et al, 2014; Khmelinskii et al, 2012). Chromosomal gene tagging and gene
deletion were performed using standard procedures based on PCR targeting as
previously described (Janke et al, 2004). Gene deletion and gene tagging were validated
by PCR. Expression of Pex13p fused to tFT tag which consists of two fluorescent
proteins mCherry and sfGFP was validated using immunoblotting and confirmed with
fluorescence microscopy.
Pex13-tFT was crossed using the synthetic genetic array method (Tong & Boone,
2006) with a yeast strain library which consisted of 152 strains that either lacked a gene
involved in protein degradation or which contained a mutant version of a protein
involved in protein degradation (in case the deletion was lethal), resulting in a library
expressing Pex13-tFT in each mutant. All the colonies used for imaging were prepared
fresh every time. WT and mutant strains expressing Pex13-tFT were first grown on YPD
plates with 2% agar at 30 °C. From agar plates, they were pinned together (Singer
Instruments) on a single plate for mating and diploid selection. Colonies were then
plated on sporulation plates (Potassium Acetate (Sigma) 20g/L, agar 2%). After
sporulation, yeast strains expressing Pex13-tFT fusions were grown at 30 °C in synthetic
complete medium (yeast nitrogen base with amino acid supplements, Sigma)
(Khmelinskii et al, 2012) with 0.1% glucose, 0.1% oleic acid, 0.5% tween and 2% agar.
The tFT library used in this study consists of one WT strain without Pex13-tFT
(used to correct the background signal), one WT with Pex13-tFT fluorescent fusion
protein (used as negative control), and 152 mutants in each of which a gene from UPS
system is disrupted either by deletion for non-essential genes or by mutations for
essential genes. Each plate had 1536 colonies, including Pex13-tFT crossed with UPS
mutants, non-functional fluorescent protein crossed with UPS mutants used for
background correction, and Pex13-tFT crossed with WT as control, with four technical
replicates for each strain. Strains were grown for 7 days, and images were taken every
day. The plates were imaged with an M1000 Pro plate reader equipped with automatic
plate loading stackers (Tecan) and custom temperature control chambers. Measurements
were taken with 10 flashes each for sfGFP (488/10nm excitation, 510/10 nm emission)
FOUR Pex13p degradation in S. cerevisiae
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and mCherry (587/10 nm excitation, 610/10 nm emission).
The mCherry/ sfGFP ratio of each mutant was the average of four colonies of the
same strain. For the further calculation of Z-score (see below), ratios of fluorescent
intensities were normalized to the WT expressing Pex13-tFT on the same plate on the
same day, and the ratio in WT expressing Pex13-tFT was set to 1.
A Z-score, also known as a standard score, indicates how many standard deviations
an element is from the mean. A Z-score can be calculated from the formula: Z= (X - μ) /
σ. In the formula, Z is the Z-score, X is the value of the element (the average of four
mCherry/ sfGFP intensity ratios of one strain on the plate on the same day), μ is the
population mean (the average of all ratios on the same plate on the same day), and σ is
the standard deviation (the standard deviation of all ratios on the same plate on the same
day). The mCherry and sfGFP fluorescence intensities were measured for colonies from
each strain on each day and the mCherry/sfGFP ratio was calculated and used to
determine the Z-score, the deviation of the ratio for a particular strain on a particular day
compared to the average ratio across all strains on that day. Increases in Z-score are
colour coded, ranging from 1.0 or less (green) to 5.0 (red). The data for each square in
the heat map are derived from four technical replicates. We applied a cut-off of 1 to
screen out most of the background. As for the interpretation of Z-scores, a Z-score less
than 0 represents an element less than the mean and a Z-score greater than 0 represents
an element greater than the mean. A Z-score equal to 1 represents an element that is one
standard deviation greater than the mean while -1 represents one standard deviation less
than the mean.
Acknowledgements
The authors thank Peter van Haastert and Maarten Linskens for helpful discussions and
Arjen Krikken for advice with processing of fluorescence microscopy images. This
work was funded by a VIDI Fellowship (723.013.004) from the Netherlands
Organisation for Scientific Research (NWO), awarded to CW.
Conflict of interest
The authors declare no conflict of interest.
Pex13p degradation in S. cerevisiae FOUR
137
Table 1, S. cerevisiae strains used in this study
Strain Description Reference
WT The SGA entry strain Y8205 (MATα
can1Δ::STE2pr-SpHIS5 lyp1Δ::STE3pr-LEU2
his3Δ1 leu2Δ0 met15Δ0 ura3Δ0) with the genetic
elements (natR) required for seamless protein
tagging, generating the library background strain
yMaM330.
(Khmelinskii
et al, 2014)
(Knop lab)
Pex11-tFT yMaM330, PEX11::mCherry-I-SceIsite-
SpCYC1term-ScURA3-I-SceIsite-mCherryΔN-sfGFP
Knop lab
Pex13-tFT yMaM330, PEX13::mCherry-I-SceIsite-
SpCYC1term-ScURA3-I-SceIsite-mCherryΔN-sfGFP
Knop lab
WT
Pex13-mGFP
Sc WT with Pex13-mGFP (zeoR) This study
WT
Pex13-mGFP+
Pex3-mKate
Sc WT with Pex13-mGFP (zeoR) and Pex3-mKate
(hygR)
This study
WT
myc-Ub-K48R+
Pex13-mGFP
Sc WT with myc tagged Ub-K8R (URA) and
Pex13-mGFP (zeoR)
This study
BY4741 MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0 (Khmelinskii
et al, 2014)
(Knop lab)
UPS deletion
library
BY4741, goi deletions::kanMX (Khmelinskii
et al, 2014)
(Knop lab)
pex2 Sc WT cell deleted PEX2 (BY4741, pex2::kanMX) Knop lab
pex2+
Pex13-mGFP
pex2 with Pex13-mGFP (zeoR) This study
pex2+
Pex13-mGFP+
Pex3-mKate
pex2 with Pex13-mGFP (zeoR) and Pex3-mKate
(hygR)
This study
pex4 Sc WT cell deleted PEX4 (BY4741, pex4::kanMX) Knop lab
pex4+
Pex13-mGFP
pex4 with Pex13-mGFP (zeoR) This study
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ufd4 Sc WT cell deleted UFD4 (BY4741, ufd4::kanMX) Knop lab
ufd4+
Pex13-mGFP
ufd4 with Pex13-mGFP (zeoR) This study
ubc4 Sc WT cell deleted UBC4 (BY4741, ubc4::kanMX) Knop lab
ubc4+
Pex13-mGFP
ubc4 with Pex13-mGFP (zeoR) This study
atg12 Sc WT cell deleted ATG12 (BY4741,atg12::kanMX) Knop lab
atg12+
Pex13-mGFP
atg12 with Pex13-mGFP (zeoR) This study
ubr2 Sc WT cell deleted UBR2 (BY4741, ubr2::kanMX) Knop lab
ubr2+
Pex13-mGFP
ubr2 with Pex13-mGFP (zeoR) This study
cdc48-3 Temperature sensitive (ts) mutant cdc48-3 contains
a heat-sensitive allele of CDC48, with permissive
(23℃) or the restrictive temperature (37℃)
(Cao et al,
2003)
cdc48-3+
Pex13-mGFP
cdc48-3 with Pex13-mGFP (zeoR) This study
cdc48-3+
Cdc5-HA6
cdc48-3 expressing Cdc5 with HA6 tag fused to its
C-terminus, hygR
This study
Table 2, plasmids used in this study
Plasmid Description Reference
pHIPZ-Pex13-mGFP C-terminal part of Pex13 fused
with mGFP, zeoR
; ampR
(Knoops et al,
2014)
pHIPH-Pex14-mKate2 Plasmid containing the C-terminal
region of H. polymorpha PEX14
fused to mKate2; hygR
; ampR
(Chen et al, 2018)
Yep Pcup1-myc-Ub-K48R Yeast episomal plasmid (URA)
containing Ub-K48R fused to myc
tag on its N-terminus, under
control of Copper ion inducible
promoter
This study
pCGCN-FAA4-mGFP Plasmid for S. cerevisiae
containing Pcup1, FAA4, mGFP,
(Saraya et al,
2010)
Pex13p degradation in S. cerevisiae FOUR
139
natR, amp
R
pRDV2 Myc tagged ubiquitin mutate
(Ub-K48R) under control of
DHAS promoter, zeoR
; ampR
(Williams & van
der Klei, 2013b)
pHIPH-Pcup1-Myc-Ub-K48R Plasmid containing myc tagged
Ub-K48R under control of CUP1
promoter, hygR
; ampR
This study
pRG226 The episomal E. coli/ S. cerevisiae
shuttle vector (empty backbone),
URA ; ampR
(Gnügge et al,
2016)
pHIPH-AID-HA6 Plasmid containing Auxin
Inducible Degron (AID) with
6xHA tag at its C-terminus, hygR
;
ampR
(Morawska &
Ulrich, 2013)
Table 3, primers used in this study
Primer Sequence Description
ScPex3-mKate-F_SRI AGCGCCAGCGTATACAG
CAACTTTGGCGTCTCCA
GCTCGTTTTCCTTCAAG
CCTATGGTTTCTGAACT
CATCAAGGA
To clone a fragment of 2858
bp containing 3’end of S.
cerevisiae PEX3 fused to
mKate with Hygromycin
resistance, forward primer,
used to make strain
Pex3-mKate
ScPex3-mKate-R_SRI TACGCTATATATATATATA
TTCTGGTGTGAGTGTCA
GTACTTATTCAGAGATTA
CGTTTTCGACACTGGAT
GGCGGC
To clone a fragment of 2858
bp containing 3’end of S.
cerevisiae PEX3 fused to
mKate Hygromycin
resistance, reverse primer,
used to make strain
Pex3-mKate
Pex3mKate-cPCR-F1 GGCAGCGTGAACGAAT
AC
To check the positive colonies
containing Pex3-mKate in the
colony PCR, forward primer
FOUR Pex13p degradation in S. cerevisiae
140
Pex3mKate-cPCR-R1 CTAGCCACTGCCACTTC
G
To check the positive colonies
containing Pex3-mKate in the
colony PCR, reverse primer
ScPex13-mGFP-F TAAAAAGACGGAAGAA
AATTGAGCATGTTGATG
ATGAAACGCGTACACAC
AGATCTGTGAGCAAGG
GC
To clone a fragment of 2240
bp containing 3’end of S.
cerevisiae PEX13 fused to
mGFP with Zeocin resistance,
forward primer, used to make
strain Pex13-mGFP
Tcyc1-dnScP13-R TAGATTTTACTATATATAT
ATGCGAATATATGTGTGC
AAATATTGATGCACTGT
ACAGAAAAAAAAGAAA
AATTTG
To clone a fragment of 2240
bp containing 3’end of S.
cerevisiae PEX13 fused to
mGFP with Zeocin resistance,
reverse primer, used to make
strain Pex13-mGFP
ScPex13-F TACGGTGCAGGAGCG To check the positive colonies
containing Pex13-mGFP in the
colony PCR, forward primer
mGFP-reverse_SRI AAGTCGTGCTGCTTCAT
GTG
To check the positive colonies
containing Pex13-mGFP in the
colony PCR, reverse primer
NotI-CUP1-F GCATGCGGCCGCCCCTT
TATTTCAGGCTGAT
To clone the 347 bp of CUP1
promoter, forward primer
CUP1-BamHI-R GTGCGGATCCTTTATGT
GATGATTGATTGATTGAT
To clone the 347 bp of CUP1
promoter, reverse primer
UbKR-SacI-R GTGCGAGCTCTCAACCA
CCTCTTAGTCTTAAG
To clone a 632 bp fragment
containing Pcup1 and
myc-Ub- K48R, reverse
primer
ScCdc5-HA6-F CTTTGATAAAGGAAGGT
TTGAAGCAGAAGTCCA
CAATTGTTACCGTAGATT
ACCCATACGATGTTCCT
GACTATGC
To clone a fragment of 1724
bp containing 3’end of S.
cerevisiae CDC5 fused to HA6
tag with Hygromycin
resistance, forward primer,
used to make strain
Cdc5-HA6, forward primer
Pex13p degradation in S. cerevisiae FOUR
141
HYG-dnCdc5-R CAATGGACTGGTAATTT
CGTATTCGTATTTCTTTC
TACTTTAATATTGGTTCG
AGATTATTCCTTTGCCCT
CGG
To clone a fragment of 1724
bp containing 3’end of S.
cerevisiae CDC5 fused to HA6
tag with Hygromycin
resistance, forward primer,
used to make strain
Cdc5-HA6, reverse primer
142
5
Chapter 5
Insights into fungal peroxisome function gained from organellar proteomics based
approaches
Xin Chen and Chris Williams
This chapter has been published as a book chapter:
Chen, X., & Williams, C. (2018). Fungal Peroxisomes Proteomics. In Proteomics of
Peroxisomes (pp. 67-83). Springer, Singapore.
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Insights into fungal peroxisome function gained from organellar proteomics based
approaches
Xin Chen and Chris Williams*
1Molecular Cell Biology, Groningen Biomolecular Sciences and Biotechnology Institute,
University of Groningen, 9747AG, the Netherlands.
*Corresponding author ([email protected])
Abstract
Peroxisomes in fungi are involved in a huge number of different metabolic processes. In
addition, non-metabolic functions have also been identified. The proteins that are present
in a particular peroxisome determine its metabolic function, whether they are the matrix
localized enzymes of the different metabolic pathways or the membrane proteins
involved in transport of metabolites across the peroxisomal membrane. Other
peroxisomal proteins play a role in organelle biogenesis and dynamics, such as fission,
transport and inheritance. Hence, obtaining a complete overview of which proteins are
present in peroxisomes at a given time or under a given growth condition provides
invaluable insights into peroxisome biology. Bottom up approaches are ideal to follow
one or a few proteins at a time but they are not able to give a global view of the content
of peroxisomes. To gain such information, top down approaches are required and one
that has provided valuable insights into peroxisome function is mass spectrometry based
organellar proteomics. Here, we discuss the findings of several such studies in yeast and
filamentous fungi and outline new insights into peroxisomal function that were gained
from these studies.
Keywords: Proteomics, Peroxisome, Fungi, Yeast, Mass spectrometry, Protein
localization
Proteomics of fungal peroxisomes FIVE
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Abbreviations:
APEX Ascorbate peroxidase
DDA Data-dependent Acquisition
DIA Data-independent Acquisition
ESI Electro-spray Ionization
GFP Green fluorescent protein
GPF Gas Phase Fractionation
ICAT Isotope-coded affinity tags
MALDI Matrix Assisted Laser Desorption Ionization
MS Mass Spectrometry
MS/MS Tandem Mass Spectrometry
µLC Micro Liquid chromatography
nHPLC High performance liquid chromatography
nLC Nano Liquid chromatography
PMP Peroxisomal membrane protein
PNS Post nuclear supernatant
PTS Peroxisomal targeting signal
ROS Reactive oxygen species
SDS-PAGE Sodium dodecyl sulfate polyacrylamide gel electrophoresis
SGD Saccharomyces cerevisiae Genome Database
SILAC Stable Isotope Labeling by Amino acids in Cell culture
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1 Introduction
Peroxisomes are eukaryotic organelles that are involved in a wide range of metabolic
functions. Some general peroxisomal functions are the oxidation of fatty acids and
detoxification of hydrogen peroxide (Smith & Aitchison, 2013b). Specific functions
include the synthesis of plasmalogens, cholesterol and bile acids in mammals (Van den
Bosch et al, 1992) while plant peroxisomes can house enzymes involved in amongst
others, the glyoxylate cycle or photorespiration (Mano & Nishimura, 2005). In this
chapter, we will discuss on fungal peroxisomes, focussing particularly on peroxisomes
in unicellular yeasts and filamentous fungi.
A very well-known species of yeast is Saccharomyces cerevisiae, which is used in the
bakery, winery and brewery industries. S. cerevisiae is also widely used as model
organism to study a huge range of biochemical, genetic and cell biological processes and
much of our understanding on the biogenesis and function of yeast peroxisomes comes
from studies in S. cerevisiae. However, the study of peroxisomes in yeast is not limited
to this organism and a plethora of data are available from studies conducted with other
yeast species, including Cryptococcus neoformans, Candida albicans, Candida boidinii,
Ustilago maydis, Yarrowia lipolytica, Hansenula polymorpha and Pichia pastoris.
Filamentous fungi are multicellular organisms that grow in a branched (filamentous)
form, termed hyphae. A number of filamentous fungi are utilized for food production,
such as certain species of Aspergillus that are used to produce Japanese Sake while
another, Penicillium chrysogenum, is used to produce penicillin, as well as a range of
bioactive secondary metabolites.
Like peroxisomes from other organisms, fungal peroxisomes also house a wide range
of metabolic pathways, allowing them to be involved in many different cellular
functions. In many yeasts, fatty acid β-oxidation takes place exclusively in peroxisomes,
as opposed to in higher eukaryotes (Kindl, 1993; Kunau et al, 1988). In this respect,
filamentous fungi are somewhat different. Aspergillus nidulans, supplementary to its
peroxisomal β-oxidation system, is able to perform β-oxidation of fatty acids in the
mitochondria (Flavell & Woodward, 1971) while the closely related Neurospora crassa
degrades fatty acids in glyoxysomes, a specialized form of peroxisome found in plants
and certain fungi (Kionka & Kunau, 1985). N. crassa (as well as several other
filamentous fungi) is particularly interesting because it contains, additional to
glyoxysomes, another specialized type of peroxisome called a Woronin body. In case of
hyphal injury, Woronin bodies act as a plug to stop leakage of the cytoplasm (Jedd &
Chua, 2000), a fascinating, non-metabolic role for peroxisomes in cell vitality. Some
additional peroxisomal functions in yeasts include the oxidation of methanol (Van
Proteomics of fungal peroxisomes FIVE
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Dijkan et al, 1982) and the metabolism of primary amines (Zwart et al, 1983) while
peroxisomes from the filamentous fungus P. chrysogenum contain the enzymes that
produce penicillin (Müller et al, 1992; Müller et al, 1991), one of the most important
drugs of all time.
2 Organellar Proteomics on Peroxisomes in Fungi
In fungi peroxisome function is extremely diverse and depends heavily on species as
well as the growth conditions. To obtain a complete understanding of the function(s) of
the peroxisome in a given cell under a given condition, a comprehensive overview of the
proteins present in these peroxisomes is crucial. The peroxisomal localization of many
metabolic pathways has been determined through bottom up approaches, using cell
fractionation methods or microscopy approaches (immunofluorescence,
immunolabelling, genetic tagging with fluorescent proteins). However, these methods
require prior knowledge of the protein in question, such as protein sequence, the
presence of targeting signals, putative function etc. and may therefore not be applicable
when the goal is to identify novel peroxisomal pathways. Furthermore, cells sometimes
house certain enzymes of a metabolic pathway in different compartments, potentially
making it a challenge to say that the localization of one protein from the pathway is
representative for the entire pathway.
Such situations call for the use of top down approaches and mass spectrometry (MS)
based proteomics methods have proved invaluable when studying the peroxisomal
proteome. Here, we summarize the findings of several MS based organellar proteomics
studies in yeast and filamentous fungi, outlining the new insights into peroxisomal
metabolism and function gained from these studies.
2.1 Organellar Proteomics on Peroxisomes from S. Cerevisiae
The earliest characterization of S. cerevisiae peroxisomes using proteomics was
performed by Schäfer et al. (Schäfer et al, 2001). Peroxisomes were isolated from oleate
grown cells through the use of differential centrifugation, followed by sucrose and
Accudenz density gradient centrifugation. Peroxisomes were lysed by osmotic shock
and peroxisomal membrane fractions were extracted and subjected to sodium dodecyl
sulphate polyacrylamide gel electrophoresis (SDS-PAGE) analysis. Following in gel
digestion, peptides were extracted and analysed with three different types of mass
spectrometry: matrix assisted laser desorption ionization (MALDI) MS, micro liquid
chromatography electrospray ionization (µLC-ESI) MS and nano liquid chromatography
ESI-MS (nLC-ESI-MS). A total of 6 known peroxisomal membrane proteins (PMPs)
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were identified, as well as 19 known peroxisomal matrix proteins, even though
peroxisomal membrane fractions were analysed. The authors did not comment further
on this aspect, but it may suggest that certain peroxisomal matrix proteins are associated
with the membrane. Indeed, a previous report suggested that the matrix protein Fat2p
(also known as Pcs60p), one of the proteins identified in this proteomics approach, is
membrane associated (Blobel & Erdmann, 1996). What this could mean in terms of
peroxisome function remains unclear.
Another interesting observation in this work was the identification of a phos-
phorylation site at Threonine 711 in the long chain fatty acid CoA ligase2 (Faa2p).
Peptides corresponding to both the phosphorylated and unphosphorylated forms were
identified, with the phosphorylated form displaying a lower signal. This could suggest
that the unphosphorylated form is the major species in vivo, although this difference in
signal intensity may be due to poor ionisation of phosphorylated peptides compared to
unphosphorylated peptides, as has been reported before (Steen et al, 2006). In a later
high throughput study, the phosphorylation status of Faa2 was confirmed (Albuquerque
et al, 2008) yet the function of this post-translational modification remains unknown.
The success of proteomics approaches is influenced by protein abundance, with
highly abundant proteins providing the majority of peptides present in a given sample,
which may in turn potentially mask lower abundant ones. Since peroxisomal matrix
proteins are likely to be much more abundant that most PMPs, approaches that regress
this balance can be extremely helpful when studying the proteome of peroxisomes. In
the above-mentioned study, Schäfer and colleagues analysed membrane fractions, rather
than whole organelles, to aid in the identification of low abundant PMPs. A similar
approach was utilised in (Yi et al, 2002). However, in order to enhance the recovery of
peptides for proteomics analysis, the authors performed tryptic digestion directly on the
isolated peroxisomal membrane fractions, rather than on gel pieces after electrophoresis.
Their approach was further enhanced through the use of gas-phase fractionation (GPF)
in combination with nLC-ESI-MS/MS. GPF relies on the separation of peptide ions in
the gas-phase of the mass spectrometer, according to their m/z value, which allows for
increased peptide coverage and reproducibility (Davis et al, 2001; Spahr et al, 2001). Yi
et al. identified 181 proteins, including 38 known peroxisomal proteins. At this time, 41
proteins were either identified or predicted to be peroxisomal, demonstrating that the
authors has a coverage of ~90% with their analysis. Of note is the identification of
Pex5p in their study. Pex5p only transiently associates with peroxisomes during the
matrix protein import cycle (Kragt et al, 2005), indicating the sensitivity of their
approach.
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While these two publications (Schäfer et al, 2001; Yi et al, 2002) clearly established
that it was possible to isolate peroxisomes for proteomics based study, they also
demonstrated one of the major drawbacks when it comes to such approaches, namely
that of contamination. Indeed, ~45% of the proteins identified in peroxisomal membrane
fractions by Schäfer et al. (2001) and ~75% of those identified in Yi et al. (2002) were
not described as peroxisomal, based on experimental evidence or prediction programs,
which raises the question whether these proteins are previously uncharacterised
peroxisomal proteins or contaminants? In the case of proteins such as the mitochondrial
membrane proteins Cyt1p and Tom40p, contamination is very probably the explanation
for their presence. However, the situation is less clear for other proteins. For example,
both studies identified Cat2p, a carnitine acetyl transferase, in their analysis. Cat2p
displays dual localisation in the peroxisome and mitochondria (Elgersma et al, 1995),
raising the question whether this protein can be considered a genuine peroxisomal
protein or a contaminant when identified in proteomics approaches? Furthermore,
Schäfer et al. classified the glycerol-3-phosphate dehydrogenase1protein (Gpd1p) as a
cytosolic contaminant while later studies demonstrated that this protein does indeed
localise to peroxisomes (see below) (Jung et al, 2010; Kumar et al, 2016; Marelli et al,
2004). Hence, methods that allow for the discrimination of contaminants from bona fide
peroxisomal proteins can aid enormously in organellar proteomics approaches by
narrowing down the number of potential peroxisomal proteins that require further
validation. With this in mind, the chapter by Islinger et al. in this book is of interest
(Islinger et al, 2018).
To tackle this, Marelli et al. utilized quantitative mass spectrometry to identify novel
peroxisomal proteins in S. cerevisiae (Marelli et al, 2004). In this study, the authors
combined isopycnic density gradient fractionation with isotope-coded affinity tags
(ICAT) to discriminate between peroxisomal proteins and contaminants. ICAT is an
approach that relies on the chemical labelling of proteins from two different fractions
with chemically identical but isotopically different tags (Gygi et al, 1999). The two
fractions are then mixed and the relative abundance of isotopically labelled peptides can
be determined using MS analysis. The relative ratio between peptides in the two
fractions will give information on whether these peptides, and hence the proteins from
which they are derived, are enriched in one fraction compared to the other. Marelli et al.
took two approaches: in the first (ICAT I), membrane fractions isolated from
peroxisomes and mitochondria derived from oleate grown cells were differentially
treated with ICAT reagents and subjected to µLC-ESI-MS/MS analysis (Fig. 1).
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Fig.1 Schematic depiction of the use of isotope-coded affinity tag (ICAT) reagents to
identify mitochondrial contaminants in peroxisomal fractions, as described in (Marelli et
al, 2004).
Peroxisomes (depicted in green) and mitochondria (in blue) were individually isolated and a
membrane fraction was prepared. Proteins isolated from the mitochondrial fraction (blue
hexagons) were treated with light ICAT reagent (red), while those isolated from the
peroxisomal fraction (green bars) were treated with heavy ICAT reagent (yellow). Next the
treated fractions were mixed and subjected to trypsin digest and mass spectrometry and the
ratio between heavy and light versions of peptides were calculated. A high heavy to light
ratio indicates that the peptide is much more abundant in the peroxisomal fraction compared
to the mitochondrial fraction, identifying this peptide as likely originating from a bona fide
peroxisomal protein. A low heavy to light ratio indicates that the peptide is not enriched in
the peroxisomal fraction, identifying it as likely contaminant.
In the second approach (ICAT II), a peroxisomal membrane fraction was isolated
from oleate grown cells that produced a Protein-A tagged version of the PMP Pex11p.
This fraction was split into two and one fraction was subjected to affinity purification
using IgG beads. Both this affinity-purified fraction, together with the untreated
membrane fraction were differentially treated with ICAT reagents and subjected to
µLC-ESI-MS/MS. ICAT I identified a total of 346 proteins, of which 23 were known
peroxisomal components according to the Saccharomyces genome database (SGD)
while 134 were described as mitochondrial. However, comparison of the relative peptide
ratios suggested that 57 of the 346 were in fact peroxisomal proteins. Of these 57, 18
were previously described as peroxisomal and none as mitochondrial, demonstrating
that the ICAT I approach can be effectively used to discriminate between genuine
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peroxisomal proteins and mitochondrial contaminants. ICAT II identified 365 proteins
but when the peptide ratios were taken into consideration, 98 proteins were suggested to
be peroxisomal, with 28 annotated as peroxisomal in the SGD. These data indicate that
ICAT II was able to identify more proteins than ICAT I, likely because the mixture was
less complex due to the affinity purification step. However, the authors state that ICAT I
would not help in identifying proteins that target to both peroxisomes and mitochondria
because such proteins would be considered mitochondrial contaminants in this approach.
ICAT II on the other hand would be able to identify such dually localised proteins but
was less efficient at identifying mitochondrial contaminants.
The authors integrated the ICAT I data into the list of 98 proteins suggested to be
peroxisomal based on the ICAT II approach and split the list of candidate proteins into
three groups. Group 1 contained 25 proteins with high peroxisomal abundance ratios
based on ICAT I. Group 2 consisted of 27 proteins with high peroxisomal abundance
ratios in ICAT I but low ratios in ICAT II. The authors concluded that these were in fact
mitochondrial contaminants. Group 3 contained 46 proteins that were predicted to be
peroxisomal in ICAT II but were not identified in ICAT I. To validate their findings the
authors tagged three proteins from Group 1 (Ybr159w, Rho1p and Faa1p) and five from
Group 3 (Erg6p, Emp24p, Gdp1p, Erg1p and Spf1p) with Protein-A and determined
their sub-cellular localisation using isopycnic density gradient fractionation. These eight
candidates were chosen because they are known to localise to different cellular
compartments, including the cytosol (Gdp1p), the ER (Spf1p, Ybr159w and Emp24p),
lipid bodies (Faa1p, Erg1p and Erg6p) and plasma/ endo-membranes (Rho1p). The
fractionation data clearly demonstrated that all eight proteins targeted partially to
peroxisomes while additional fluorescence microscopy analysis of green fluorescent
protein (GFP) fusions of Rho1p, Gdp1p and Emp24p further confirmed that these
proteins can partially localise to peroxisomes. The localisation of Erg1p-GFP was
unclear but appeared to be close to peroxisomes.
Localisation is one thing, but the question remained as to what the function of these
proteins in or at peroxisomes could be. To address this aspect, the authors chose to study
the role of Rho1p, a small, ras-related GTPase, in peroxisome biology. Rho1p functions
in signal transduction and has been shown to regulate actin reorganisation (Fujiwara et
al, 1998; Nonaka et al, 1995; Yamochi et al, 1994). The authors demonstrated that
Rho1p targets to peroxisomes in cells grown on oleate and not on glucose, which led
them to suggest that the reason Rho1pwas not previously localised to peroxisomes was
because most studies of Rho1p were performed with glucose grown cells. Peroxisomes
were smaller and lower in number in cells containing a temperature sensitive mutant
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form of rho1 while Rho1p interacts with the peroxisome biogenesis factor Pex25p and
requires Pex25p for its peroxisomal localisation, suggesting a link between Rho1p and
peroxisome fission/ biogenesis. Finally, the authors demonstrated that actin disassembly
at peroxisomes is controlled by Rho1p and Pex25p, leading to the suggestion that Rho1p
plays a role in peroxisome fission by dissembling actin at fission sites in order to allow
Pex11p and other proteins involved in peroxisomal fission to finalise the fission event.
Taken together, this report elegantly demonstrates that quantitative proteomics can be
used to identify previously unknown peroxisomal proteins in order to shed new light
onto peroxisome biogenesis.
It is worthy to note here that isotope labelling of proteins can also be performed
metabolically, using a method called Stable Isotope Labelling by Amino acids in Cell
culture (SILAC). Rather than using a chemical approach to modify proteins or peptides
after isolation, as ICAT does, SILAC relies on the cells themselves to incorporate the
isotopically labelled amino acids Lysine and Arginine residues into proteins. Cells are
grown in the presence of “heavy” or “light” versions of these amino acids, samples are
mixed and subjected to MS and the relative ratios of the heavy and light forms of the
peptides can be used to identify contaminants. Although this method has not been used
in organellar proteomics on fungi, it has been successfully used when investigating the
interaction partners of yeast peroxisomal proteins (David et al, 2013; Oeljeklaus et al,
2012; Piechura et al, 2012).
Because peroxisomes are metabolic organelles, the protein content of peroxisomes
depends very much on the metabolic needs of the cell. Peroxisomes contain an import
system that can react to the metabolic needs of the cell (Nonaka et al, 1995; Yifrach et al,
2016), which means that peroxisomal protein content is dynamic and condition specific.
Measuring the change in subcellular localisation with bottom up approaches such as live
cell imaging can provide invaluable information on the dynamic properties of a given
protein. However, such properties are challenging to measure in top down approaches
that seek to characterise global changes in protein localisation. One reason for this is the
difficulty that is encountered when comparing samples of different origins, such as
peroxisomes isolated from cells grown on glucose compared to peroxisomes isolated
from cells grown on oleate. Classical MS approaches often rely on the data-dependent
acquisition (DDA) method, a semi-random process that effectively selects ionized
peptides with high signal to noise ratios for further analysis. Because of this, ions of low
signal to noise ratio may be “ignored” by the detector. Hence, a given peptide ion may
have a low signal to noise ratio in one sample, meaning that it is underrepresented, while
the same peptide ion may have a high signal to noise ratio in another sample, meaning
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that it is overrepresented. Because of this bias in sampling, valuable data may become
lost. To address this issue, Jung et al. (2010) employed a data independent acquisition
(DIA) approach to investigate global differences in protein distribution in cells grown on
glucose compared to those grown on oleate. Although they did not focus on peroxisomes
in this report, their data did elegantly demonstrate that protein redistribution can occur
on many different levels. Enzymes involved in metabolic processes associated with fatty
acid processing underwent strong upregulation and redistribution to organelles in
response to exposure to oleate whereas proteins involved in peroxisomal organisation
(such as the docking factors Pex3p and Pex14p) also redistributed to organelles in
response to oleate treatment yet they were not strongly upregulated. While this may not
seem surprising at first glance, it does provide a very interesting insight into the
behaviour of these different classes of proteins on a global scale and it also provides a
benchmark that can be utilised to assess the role of proteins with unknown functions.
2.2 The Proteome of Peroxisomes in N. Crassa
The filamentous fungus N. crassa possesses two types of peroxisomes: glyoxysomes and
Woronin bodies. Glyoxysomes in N. crassa, like peroxisomes in many organisms, house
enzymes required for β-oxidation. However, they also contain enzymes of the glyoxylate
cycle, a metabolic pathway that allows for the conversion of acetyl-CoA to succinate,
which is then used further for carbohydrate production (Flavell & Woodward, 1971).
The β-oxidation pathway in glyoxysomes is somewhat different from that in other yeasts.
Rather than relying on an acyl-CoA oxidase to perform the dehydration of the fatty
acyl-CoA species, the first step in the β-oxidation pathway, glyoxysomes instead use
acyl-CoA dehydrogenase to perform this function. This alternative mechanism does not
generate hydrogen peroxide and subsequently, glyoxysomes from N. crassa do not
contain catalase, the major detoxifier of hydrogen peroxide in peroxisomes (Schliebs et
al, 2006). Woronin bodies, on the other hand, perform a non-metabolic function. They
stop the loss of cytoplasm upon hyphal injury by acting as a plug (Jedd & Chua, 2000).
Interestingly, Woronin bodies seem to form from glyoxysomes. First the protein
Hexagonal 1 (HEX1) is imported to glyoxysomes through its Peroxisomal targeting
signal type 1 (PTS1), after which it forms a large, hexagonal crystal. The Woronin body,
complete with HEX1 crystal, then buds off from the glyoxysome through fission (Liu et
al, 2008; Managadze et al, 2007).
In order to gain a better understanding of the protein content of these two specialized
forms of peroxisomes, Managadze et al. performed organellar proteomics upon isolated
glyoxysomes and Woronin bodies from N. crassa (Managadze et al, 2010). Woronin
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bodies were purified from a post nuclear supernatant (PNS) isolated from sucrose grown
cells through the use of a linear sucrose gradient. Samples were subjected to SDS-PAGE
and fractions that contained the most amount of the Woronin body marker protein HEX1
and the least amount of glyoxysomal and mitochondrial contaminants were pooled and
subjected to SDS-PAGE and coomassie staining. The authors observed 15 protein bands
on the gel after these steps and these 15 bands were excised, subjected to in-gel
digestion and peptides were analysed by nano High-Performance Liquid
Chromatography (nHPLC) ESI-MS/ MS. As could be expected, the major component
identified was HEX1. The authors did identify a number of additional proteins but since
these corresponded to ribosomal and mitochondrial proteins, they concluded that these
likely represented contaminants. However, this approach did identify NCU00627, a
protein of unknown function with homologues in other filamentous fungi. Whether this
is a bona fide Woronin protein and if so, what its role might be, are questions that remain
to be answered.
The authors had more luck with their organellar proteomics approach on glyoxysomes.
Glyoxysomes were isolated from a PNS derived from oleate grown cells and subjected
to “density barrier centrifugation”. In this approach, the organellar pellet was mixed
with iodixanol to a final concentration of 23.5% and this mix was layered onto a denser
solution of iodixanol (35%). After centrifugation, glyoxysomes concentrate at the
interface between the two densities; the “barrier”. Glyoxysomes were then disrupted
with SDS and heating and the resulting protein fraction was subjected to reverse phase
chromatography, SDS-PAGE analysis and coomassie staining. Visible protein bands
were excised and subjected to in gel digestion and the peptides were analysed by
nHPLC-ESI-MS/MS. This approach led to the identification of 191 proteins. Amongst
this list, the authors noted that 16 proteins contained a putative PTS1 sequence while 3
contained a putative PTS2 sequence and although the rest lacked a recognisable
targeting sequence, they noted a number of proteins that were functionally linked to
glyoxysomes, such as isocitrate lyase (ICL), which was shown to be peroxisomal in
Aspergillus nidulans (Valenciano et al, 1998).
The authors validated their results through the use of fluorescence microscopy,
showing that three candidates from the list of PTS1 proteins indeed targeted to
peroxisomes. The three proteins they chose were NCU02287, NCU08924 and
NCU04803. The first two are putative acyl-CoA dehydrogenases (which the authors
named ACD1 and ACD2) and confirmation of their glyoxysomal localisation was
significant because up until this point, the identity of the acyl-CoA dehydrogenase
required for β-oxidation in glyoxysomes was unknown. Interestingly, the authors also
Proteomics of fungal peroxisomes FIVE
155
identified a fumarate reductase homologue in the list of the 191 putative glyoxysomal
proteins. As mentioned, the first step of β-oxidation in glyoxysomes is a dehydration
reaction, performed by acyl-CoA dehydrogenase. The authors speculate that this
fumarate reductase enzyme could be involved in the re-oxidation of the co-factor that is
required by acyl-CoA dehydrogenase.
The third candidate which the authors tagged with GFP for localisation studies was a
2-nitropropane dioxygenase (now referred to as nitronate monooxygenase), which they
named NPD1. Another protein (NCU09931), which possessed similar domain structure
as well as a PTS1, was identified in the proteomics screen. The authors termed this
candidate NPD2 and propose that these enzymes are involved in the detoxification of
nitroalkanes, which may play a role in protecting N. crassa against nitroalkanes excreted
by other organisms (Alston et al, 1977; Hipkin et al, 1999). Taken together, these data
identified a novel enzymatic activity housed within peroxisomes, expanding the role of
peroxisomes in cell metabolism.
2.3 Identification of Peroxisomal Matrix Proteins in P. Chrysogenum
Peroxisomes in the filamentous fungus P. chrysogenum are important to the medical and
industrial sectors because they house the enzymes that produce penicillin (Müller et al,
1992; Müller et al, 1991). With this in mind, knowledge on the protein content of
peroxisomes in this organism can help in understanding how penicillin and other
secondary metabolites are produced. This led Kiel and colleagues to investigate the
proteome of peroxisomes in P. chrysogenum (Kiel et al, 2009). Peroxisomes were
isolated with a sucrose density gradient from a PNS, lysed by osmotic shock and the
matrix protein fraction was analysed by SDS-PAGE, coomassie staining and in-gel
digestion. The subsequent peptide mix was subjected to nHPLC-MS/MS, leading to the
identification of more than 500 proteins. A significant portion of these (119) were
involved in translation, which could represent a large amount of ribosomal
contamination. However, the authors demonstrated with electron microscopy analysis
that ribosomes sometimes associated with isolated peroxisomes. The authors therefore
suggested that rather than representing contamination, these may be ribosomes
translating peroxisomal proteins at the peroxisomal membrane. Since this study, Zipor et
al. demonstrated that mRNA translation of peroxisomal proteins can indeed occur in
close proximity to peroxisomes in S. cerevisiae (Zipor et al, 2009), which could validate
the authors theory.
The remaining proteins were manually annotated and classified based on their
potential localisation within the cell and the authors listed a total of 89 putative
FIVE Proteomics of fungal peroxisomes
156
peroxisomal proteins. Many proteins contained a PTS1 (69) while 10 more contained a
putative PTS2, strongly suggesting that they indeed target to peroxisomes. A further 10
proteins that lacked a PTS were deemed likely to be peroxisomal, either because they
were particularly abundant in the preparation, because of function (e.g. several were
involved in b-oxidation, which is often a peroxisomal process) or because of previous
data on their localisation, such as ICL (see above).
Of the 89 putative peroxisomal proteins, many were enzymes that take part in
metabolic pathways, such as penicillin production, fatty acid β-oxidation, the glyoxylate
cycle and nitrogen metabolism. Furthermore, a number of enzymes involved in the
detoxification of ROS were identified, as were several thioesterases. Finally, the
peroxisomal role of around 35 of the 89 enzymes identified in the approach was not
clear from their putative function, which was defined by their homology to other
enzymes. It is worthy to note that the authors identified one acyl-CoA oxidase and four
acyl-CoA dehydrogenases in their proteomic approach. As mentioned, fatty acid
β-oxidation generates hydrogen peroxide when acyl-CoA oxidase catalyses the first step
in the cascade whereas this is not the case when the first step is catalysed by acyl-CoA
dehydrogenase. This high number of acyl-CoA dehydrogenases could suggest that fatty
acid β-oxidation occurs via a dehydration step in P. chrysogenum peroxisomes. In
support of this, the author also identified a Fumarate reductase homologue (Pc12g0390)
in their proteomic approach and confirmed its localisation using GFP tagging and
fluorescence microscopy. This enzyme may play a role in the re-oxidation of co-factors
required by acyl-CoA dehydrogenase for fatty acid β-oxidation, as was suggested for the
N. crassa orthologue (see above). However, the authors also identified several catalase
like enzymes in their proteomics approach, indicating that P. chrysogenum peroxisomes
are a likely site of hydrogen peroxide production. Furthermore, later studies
demonstrated that additional acyl-CoA oxidases target to peroxisomes and that these
enzymes are involved in fatty acid β-oxidation (Veiga et al, 2012). Clearly further
studies are required to investigate the intricate nature of peroxisomal fatty acid
β-oxidation in P. chrysogenum.
The wide range of functions displayed by the 89 putative peroxisomal proteins led the
authors to conclude that peroxisomes in P. chrysogenum are not simply penicillin
production factories but are instead multi-purpose organelles that house many different
metabolic pathways. Nevertheless, since the peroxisomes used in this study were
isolated from cells growing on media that stimulates the production of penicillin, these
data laid down a solid basis for further study into the role of peroxisomes in the
production of penicillin.
Proteomics of fungal peroxisomes FIVE
157
3 Perspectives
Advances in the sensitivity and speed of mass spectrometers, the development of
methods to identify contaminants, as well as in statistical methods to analyse the huge
amount of data generated by these approaches have allowed organellar proteomics to
make invaluable contributions to peroxisomal research. However, a number of PMPs are
relatively low in abundance (Reguenga et al, 2001), making their detection using MS
still tricky, while it remains a challenge to investigate proteins displaying a dual
localisation using MS because the issue of contamination still arises (Schäfer et al, 2001;
Yi et al, 2002). Finally, the preparation of peroxisomal fractions for MS analysis remains
a long and often challenging process (as discussed in (Islinger et al, 2018; Saleem et al,
2006)). Because the success of an organellar proteomics approach depends heavily on
the quality and purity of the samples being analysed, we will end by discussing two
recent developments that may allow isolation procedures for future MS based studies to
be simplified.
Recently, Peikert et al. Reported a method they termed ImportOmics, which relies on
RNA inhibition (RNAi) of the docking factor Pex14p in the parasite T. brucei (Peikert et
al, 2017). The inhibition of Pex14p production blocked the import of matrix proteins
into the glycosome, a specialized type of peroxisome involved in the breakdown of
glucose in this organism (Bauer & Morris, 2017). The authors elegantly demonstrated
that matrix proteins became mistargeted in cells where Pex14p was targeted with RNAi,
allowing them to directly compare the levels of certain proteins in the organellar pellet
fraction of untreated cells versus an organelle pellet isolated from cells where Pex14p
was targeted. This was possible using a simple differential centrifugation approach,
negating the requirement for density centrifugation and greatly shortening and
simplifying the isolation procedure. Although RNAi has not been used extensively in
yeast or filamentous fungi, alternative approaches such as the Degron based system have
been used successfully to down-regulate peroxisomal proteins (Knoops et al, 2015;
Motley et al, 2015; Nuttall et al, 2014), which would allow such experiments to be
performed in these organisms. Furthermore, the authors noticed that blocking the import
of proteins into mitochondria through the same RNAi based approach not only resulted
in mitochondrial protein mistargeting to the cytosol but also to their proteasomal based
degradation, allowing the authors to gain information on whether a given protein targets
to the mitochondria or not based on their absolute levels in total cell lysates. Therefore
the authors could identify proteins that target to mitochondria using a single step
isolation procedure. While this may not be applicable for peroxisomal matrix proteins,
FIVE Proteomics of fungal peroxisomes
158
because proteasomal degradation of mistargeted matrix proteins has not, to the best of
our knowledge, been reported for yeast matrix proteins, this would certainly be an
interesting possibility when PMPs are being studied. Several PMPs are degraded when
mistargeted (Knoops et al, 2014) meaning that in principle downregulating Pex19p, the
receptor protein for PMPs (Neufeld et al, 2009; Rucktaschel et al, 2009), would result in
decreased levels of proteins that require Pex19p for targeting to peroxisomes. This could
allow for the identification of novel PMPs using a single step isolation procedure.
Fig.2 Schematic depiction of in vivo proximity labelling of proteins using an engineered
form ascorbate peroxidase (APEX).
Targeting of APEX to an organelle will result in the modification of proteins present in the
organelle. APEX converts biotin-phenol substrates into highly reactive biotin-phenol radicals
that become covalently attached to neighbouring proteins on tyrosine residues. Following
cell lysis, modified proteins can be extracted using streptavidin beads (if required, under
denaturing conditions), the samples can be subjected to trypsin digest and the resulting
peptides can be analysed with mass spectrometry.
The second development we mention concerns the use of proximity labelling, a
chemical biology based approach that utilises a labelling enzyme to modify proteins
with an affinity tag in vivo (Kim & Roux, 2016). This affinity tag can then be employed
to fish out modified proteins for further analysis. Targeting the labelling enzyme to a
particular compartment (through the use of a targeting signal or by fusing it to an
abundant protein present in that compartment) results in the specific modification of
proteins in that compartment (Fig. 2). A commonly used labelling enzyme is an
engineered version of ascorbate peroxidase (APEX) from plants (Martell et al, 2012)
Proteomics of fungal peroxisomes FIVE
159
and this enzyme was successfully employed by Rhee and co-workers to identify novel
mitochondrial proteins in mammalian cells (Rhee et al, 2013). Another recent report
demonstrated that a similar system can be used in yeast (Hwang & Espenshade, 2016).
APEX oxidizes biotin-phenol in the presence of hydrogen peroxide, which generates
short-lived biotin-derivative radicals that can covalently react with tyrosine residues in
proteins in the near vicinity. Both biotin-phenol and hydrogen peroxide are added
externally, meaning that the amount as well as the time at which protein labelling occurs
can be regulated. Because the isolation of organelles is not required, proteins (or
peptides resulting from tryptic digestion) modified with biotin can be isolated directly
from cell lysates with streptavidin beads and analysed by MS, speeding up and
simplifying extraction procedures. Furthermore, since streptavidin can bind to biotin
under denaturing conditions, the isolation of biotinylated proteins can be performed
under denaturing conditions, which dramatically reduces the loss of material due to the
action of cellular proteases. Finally, such approaches have the potential to identify
transient residents of an organelle, which is still highly challenging with alternative
approaches (Jung et al, 2010). Needless to say, we eagerly await the first report on the
use of proximity labelling in the study of the proteome of fungal peroxisomes.
To conclude, the use of organellar proteomics to study fungal peroxisomes has
provided valuable insights into the role of peroxisomes in the cell. The new
developments listed above, together with others not mentioned here, will help to make
isolation procedures both quicker and easier, allowing organellar proteomics approaches
to continue to make important contributions to the study of peroxisome function in the
future.
Acknowledgements C.W. is supported by a VIDI Grant (723.013.004) from the
Netherlands Organization for Scientific Research (NWO).
References
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188
6
Chapter 6
Summary and Discussion
Xin Chen and Chris Williams
SIX Summary
190
Summary and Discussion
Peroxisomes are single membrane bound organelles found in nearly all eukaryotic cells.
Peroxisomes participate in a variety of biological processes, including fatty acid
β-oxidation, the glyoxylate cycle, plasmalogens synthesis, photorespiration and purine
biosynthesis. The function of a peroxisome is determined by the matrix proteins (MATs)
in the peroxisomal lumen, often involved in metabolism and peroxisomal membrane
proteins (PMPs), which are involved in the transport of proteins and small molecules
into peroxisomes, peroxisomal fission and the interplay between peroxisomes and other
organelles. Because peroxisomes post-translationally import all the proteins required for
function, protein transport processes play an important role in defining peroxisome
function. However, at some point during their lifetime, all proteins in the cell undergo
protein degradation. Hence, protein degradation can also be expected to impact on
peroxisomal function. Protein degradation may occur because they are “worn out” by
chemical modifications, because they become unfolded or because they are no longer
needed. Protein degradation needs to be regulated, otherwise unwanted degradation
events may occur or unwanted proteins start to build up in the cell. Understanding how
and why proteins are degraded allows us to better understand the role of protein
degradation in a cellular context.
The ubiquitin-proteasome system (UPS) plays an important role in protein turnover
in many cellular processes, including the cell cycle, the regulation of gene expression
and responses to oxidative stress. The UPS involves the attachment of the 8 kDa protein
ubiquitin (Ub) to a substrate protein in an ATP dependent process, requiring three
distinct enzymes. First, the ubiquitin activating enzyme (E1) activates ubiquitin. Next,
the activated ubiquitin is transferred to the active site cysteine residue of an ubiquitin
conjugating enzyme (E2). Finally, an ubiquitin ligase (E3) allows conjugation of
ubiquitin to the substrate. The ubiquitin attached to the substrate can itself become a
substrate for ubiquitination, resulting in the formation of ubiquitin chains. Such Ub
chains can target substrates for degradation via the proteasome.
Peroxisomes have their own, membrane-associated ubiquitination machinery,
consisting of the ubiquitin conjugating enzyme Pex4p in yeast (or member of the Ube2D
E2 family in mammals) and an E3 ligase complex, containing the RING proteins Pex2p,
Pex10p and Pex12p. The peroxisomal ubiquitination machinery is mostly known for the
ubiquitination of the cycling receptor proteins Pex5p and Pex20p family members.
However, the role of the peroxisomal ubiquitination machinery in peroxisome function
is still not well understood while, unlike other organelles, next to nothing is known
Summary SIX
191
about how PMPs are targeted for degradation. The research described in this thesis
aimed to investigate how and why PMP degradation occurs. Our study focuses on the
degradation of the PMP Pex13p in yeast and the corresponding function of Pex13p
degradation in the context of peroxisome biology and cellular metabolism.
In Chapter one, we present an overview of cellular processes that regulate
peroxisome function, ranging from how peroxisomes are made to how they are degraded.
Furthermore, we discuss the current knowledge on how membrane proteins present on
organelles undergo degradation, the role of the UPS in membrane protein degradation
and finally how PMP degradation may be facilitated.
In Chapter two, we show that the PMP Pex13p undergoes rapid turnover in H.
polymorpha wildtype cells and describe a role of the peroxisomal ubiquitination
machinery in Pex13p turnover. We establish that Pex13p is ubiquitinated in wildtype
cells and that the ubiquitination of Pex13p is reduced in the absence of a functional
peroxisomal E3 ligase complex. Furthermore, cells lacking members of this machinery
display elevated level of Pex13p and accumulate Pex13p at the peroxisomal membrane.
Our results add strong support to the idea that the peroxisomal ubiquitination machinery
is not only required for ubiquitinating Pex5p and members of the Pex20p family but also
targets additional peroxisomal proteins. When taken together, we now know that
members of the peroxisomal E3 ligase complex are involved in the ubiquitination/
degradation of Pex5p and Pex20p, the PMP Pex3p in H. polymorpha and in the
ubiquitination of PMP70 in mammals. This suggests a ubiquitous and important role for
the peroxisomal ubiquitination machinery in peroxisomal proteins
ubiquitination/degradation as well as in peroxisome biology.
In Chapter three, we investigate the potential functions of Pex13p degradation in
the yeast H. polymorpha. We demonstrated that Pex2p-dependent turnover of Pex13p
also occurs under peroxisome non-inducing condition, demonstrating that Pex13p
degradation is a general and not a condition-specific event. We also show that blocking
the recycling of Pex5p inhibits Pex13p degradation, indicating that the removal of
Pex5p from the peroxisomal membrane is linked to Pex13p degradation. Furthermore,
we identify a mutant form of Pex13p that is inhibited in degradation and establish that
blocking Pex13p degradation can negatively impact on peroxisome function in vivo.
Finally, we demonstrate that Pex13p levels increase in cells overproducing Pex14p,
suggesting that Pex13p degradation is reduced in these cells and that Pex13p
degradation is dependent on Pex14p levels. Taken together, these observations strongly
suggest an important coupled relationship between Pex13p degradation and the import
of matrix proteins into peroxisomes. It is possible that Pex13p degradation negatively
SIX Summary
192
regulates matrix protein import by disconnecting the docking complex (of which Pex13p
is a member) from the downstream components required for the recycling of the PTS1
protein import receptor Pex5p, such as the RING E3 complex or the AAA-ATPases
Pex1p and Pex6p. However, since Pex13p degradation is a rapid and general event that
occurs under different growth conditions, the notion that Pex13p degradation negatively
regulates matrix protein import might seem unlikely. Another hypothesis is that Pex13p
degradation is required to dissociate the transient importomer complex. The rapid
association and dissociation of multiple factors in the importomer complex is likely
required for the import process and it could be envisaged that removal of Pex13p out of
the importomer complex may destabilize the importomer and lead to the release of cargo
proteins into the lumen or alternatively to the recycling Pex5p to the cytosol. Hence,
further work that addresses the role of Pex13p degradation in matrix protein import is
required.
In Chapter four, we have investigated Pex13p degradation in the yeast S.
cerevisiae and utilized a tandem fluorescent protein timer (tFT) to identify additional
factors involved in Pex13p degradation. Our data demonstrate that Pex13p rapid
degradation is conserved in S. cerevisiae wild type cells grown on oleic acid media and
that Pex13p is degraded via UPS, again establishing that Pex13p turnover is likely to
play an important role in peroxisome biology. In addition, the peroxisomal
ubiquitination machinery plays a major role in Pex13p turnover, while the additional
cytosolic UPS factors Ufd4p, Ubc4p and Ubr2p play a minor role in Pex13p turnover,
possibly through the formation of poly-ubiquitin chains on Pex13p. The fact that
multiple E2s and E3s appear to play a role in Pex13p degradation suggests that either
several pathways act in parallel on Pex13p to facilitate its degradation or that all these
factors act together in ubiquitinating Pex13p, to target the protein for proteasomal
degradation. Furthermore, these observations indicate that cytosolic UPS factors can
regulate the turnover of PMPs and hence have the potential to impact on peroxisome
function. This, in turn, indicates that the degradation of PMPs, like that of ER and
mitochondrial membrane proteins, is regulated at the level of the general cellular protein
degradation pathways. Finally, our data also demonstrate that the function of Cdc48p is
not required for Pex13p degradation. Since Cdc48p is involved in the degradation of ER
and mitochondrial membrane proteins, this observation sets the degradation of PMPs
apart from that of other organellar membrane proteins and establishes that different
mechanisms exist to facilitate these degradation processes. One possibility is that the
AAA-ATPases Pex1p and Pex6p, which are involved in the extraction of ubiquitinated
Pex5p from the peroxisomal membrane, target ubiquitinated Pex13p to the proteasome.
Summary SIX
193
However, the membrane bound AAA-ATPase Msp1p, which was reported to extract tail
anchored proteins out of the peroxisomal membrane for degradation, can also be seen as
an interesting candidate for further study. Finally, recent reports indicate that the
proteasome can be recruited to membranes to facilitate the degradation of membrane
proteins. Perhaps such a mechanism also controls the degradation of Pex13p. Clearly
further work is needed to investigate how ubiquitinated Pex13p is extracted from the
peroxisomal membrane.
Peroxisome function is extremely diverse and depends on species, cell type and
growth conditions. In order to have a complete understanding of the function(s) of
peroxisomes in a given cell under a given condition, a complete overview of the proteins
present in these peroxisomes is vital. Mass spectrometry based proteomics methods have
proved invaluable when studying the peroxisomal proteome and have provided several
new and novel insights into peroxisome function. In Chapter five we have summarize
the findings of several mass spectrometry-based organellar proteomics studies in yeast
and filamentous fungi and have outlined the new insights into peroxisomal function
gained from the studies.
PMPs are involved in all peroxisomal functions and therefore are vitally important for
cellular metabolism. The further study of PMP degradation will greatly enhance our
understanding of how PMP homeostasis is maintained and how this impacts on
peroxisome function. In this thesis we have investigated the degradation of the PMP
Pex13p in yeast and the contribution of the peroxisomal membrane ubiquitination
machinery, as well as additional components of the UPS, in this process. The fact that
Pex13p undergoes degradation in two different organisms, apparently via similar
mechanisms, strongly suggests that the ability to degrade Pex13p is both a general trait
of peroxisomes and that it is important for the function of Pex13p in the matrix protein
import process. Going one step further, should Pex13p degradation also occur in
mammalian cells, this raises the question how Pex13p degradation may contribute to
human health and whether defects in Pex13p degradation have the potential to cause
human disease. Furthermore, because Pex13p degradation in both organisms requires
the peroxisomal ubiquitination machinery, coupled with previous reports that
demonstrate a role for members of this machinery in the ubiquitination and degradation
of additional PMP, we suspect that the peroxisomal ubiquitination machinery is in fact a
general ubiquitination platform present on the peroxisomal membrane that targets
multiple substrates. Future studies that aim to identify additional substrates of this
machinery will provide invaluable new insights into the role of the machinery in
peroxisomal function.
194
Samenvatting
195
Samenvatting
Peroxisomen zijn enkelmembraan-gebonden organellen die in bijna alle eukaryote cellen
worden aangetroffen. Peroxisomen nemen deel aan een verscheidenheid van biologische
processen, waaronder vetzuur-β-oxidatie, de glyoxylatie cyclus, plasmalogen synthese,
fotorespiratie en purinebiosynthese. De functie van een peroxisoom wordt bepaald door
de matrixeiwitten (MAT's) in het peroxisomale lumen, vaak betrokken bij het
metabolisme, en door de peroxisomale membraaneiwitten (PMP's), die betrokken zijn
bij het transport van eiwitten en kleine moleculen naar peroxisomen, de deling van
peroxisomen en het samenspel tussen peroxisomen en andere organellen. Omdat
peroxisomen alle eiwitten die nodig zijn voor functie post-translationeel importeren,
spelen eiwittransportprocessen een belangrijke rol bij het definiëren van de
peroxisoomfunctie. Alle eiwitten in de cel worden echter ook op enig moment tijdens
hun levensduur afgebroken. Van eiwitafbraak kan daarom ook worden verwacht dat
deze invloed heeft op de peroxisomale functie. Eiwitafbraak kan optreden omdat
eiwitten "versleten" zijn door chemische modificaties, omdat ze ontvouwen worden of
omdat ze niet langer nodig zijn. Eiwitafbraak moet zorgvuldig worden gereguleerd,
anders kunnen ongewenste afbraakgebeurtenissen optreden of beginnen ongewenste
eiwitten zich in de cel op te hopen. Door te begrijpen hoe en waarom eiwitten worden
afgebroken, kunnen we de rol van eiwitafbraak in een cellulaire context beter begrijpen.
Het ubiquitine-proteasome systeem (UPS) speelt een belangrijke rol bij
eiwitomzetting in veel cellulaire processen, waaronder de celcyclus, de regulatie van
genexpressie en reacties op oxidatieve stress. De UPS zorgt voor de koppeling van het 8
kDa eiwit ubiquitine (Ub) aan het af te breken eiwit in een ATP-afhankelijk proces,
waarbij drie verschillende enzymen zijn vereist. Eerst activeert het
ubiquitine-activerende enzym (E1) ubiquitine. Vervolgens wordt het geactiveerde
ubiquitine overgebracht naar het cysteïne residu in de actieve plaats van een
ubiquitine-conjugerend enzym (E2). Ten slotte maakt een ubiquitine-ligase (E3)
conjugatie van ubiquitine aan het substraat mogelijk. Het ubiquitine gehecht aan het
substraat kan zelf een substraat worden voor verdere ubiquitinatie, resulterend in de
vorming van ubiquitine ketens. Dergelijke Ub-ketens kunnen substraten markeren voor
degradatie via het proteasoom.
Peroxisomen hebben hun eigen membraangeassocieerde ubiquitinatie-machinerie,
bestaande uit het ubiquitine-conjugatie-enzym Pex4p in gist (vergelijkbaar met de
Ube2D E2-familie in zoogdieren) en een E3-ligasecomplex, dat de RING-eiwitten
Pex2p, Pex10p en Pex12p bevat. De peroxisomale ubiquitinatie-machinerie is het meest
Samenvatting
196
bestudeerd bij de ubiquitinatie van de cyclische receptoreiwitten uit de Pex5p en
Pex20p-familie. De rol van de peroxisomale ubiquitinatie-machinerie in de
peroxisoomfunctie wordt echter nog steeds niet goed begrepen, terwijl er, in
tegenstelling tot andere organellen, bijna niets bekend is over hoe PMP's worden
gemarkeerd voor afbraak. Het onderzoek beschreven in dit proefschrift heeft als doel na
te gaan hoe en waarom afbraak van PMP optreedt. Onze studie richt zich op de afbraak
van de PMP Pex13p in gist en de functie van deze Pex13p afbraak in de context van
peroxisoombiologie en cellulair metabolisme.
In Hoofdstuk een presenteren we een overzicht van cellulaire processen die de
peroxisoomfunctie reguleren, van hoe peroxisomen worden gemaakt tot hoe ze worden
afgebroken. Verder bespreken we de huidige kennis over hoe membraaneiwitten van
organellen worden afgebroken, de rol van de UPS in afbraak van membraaneiwitten en
tenslotte hoe PMP-degradatie mogelijk kan worden gemaakt.
In Hoofdstuk twee laten we zien dat de PMP Pex13p een snelle turnover ondergaat
in H. polymorpha wildtype cellen en we beschrijven een rol van de peroxisomale
ubiquitinatie-machinerie in Pex13p-turnover. We stellen vast dat Pex13p
ge-ubiquitineerd is in wildtype cellen en dat de ubiquitinering van Pex13p is verminderd
in de afwezigheid van een functioneel peroxisomaal E3-ligasecomplex. Bovendien
vertonen cellen die componenten van deze machinerie missen een verhoogd niveau van
Pex13p en in deze cellen accumuleert Pex13p aan het peroxisomale membraan. Onze
resultaten ondersteunen het idee dat de peroxisomale ubiquitinatie-machinerie niet
alleen nodig is voor het ubiquitineren van Pex5p en eiwitten van de Pex20p-familie,
maar ook gericht is op andere peroxisomale eiwitten. Samenvattend, weten we nu dat
componenten van het peroxisomale E3-ligasecomplex betrokken zijn bij de
ubiquitinatie/afbraak van Pex5p en Pex20p, het PMP Pex3p in H. polymorpha en bij de
ubiquitinering van PMP70 bij zoogdieren. Dit suggereert naast een universele en
belangrijke rol voor de peroxisomale ubiquitinatie-machinerie bij ubiquitinatie/afbraak
van peroxisomale eiwitten ook een rol in peroxisomale biologie.
In Hoofdstuk drie onderzoeken we de mogelijke functies van Pex13p afbraak in
de gist H. polymorpha. We hebben aangetoond dat de Pex2p-afhankelijke turnover van
Pex13p ook optreedt onder peroxisoom niet-inducerende omstandigheden, wat aantoont
dat degradatie van Pex13p een algemene, en geen conditie-specifieke, gebeurtenis is. We
laten ook zien dat het blokkeren van de recycling van Pex5p de afbraak van Pex13p remt,
wat aangeeft dat de verwijdering van Pex5p uit het peroxisomale membraan is
gekoppeld aan degradatie met Pex13p. Verder identificeren we een gemuteerde vorm
van Pex13p die wordt geremd bij afbraak en we stellen vast dat blokkering van Pex13p
Samenvatting
197
afbraak een negatieve invloed kan hebben op de peroxisoomfunctie in vivo. Tenslotte
tonen we aan dat Pex13p-niveaus toenemen in cellen die Pex14p overproductie vertonen,
wat suggereert dat afbraak van Pex13p in deze cellen is verminderd en dat degradatie
van Pex13p afhankelijk is van Pex14p-niveaus. Samenvattend suggereren deze
waarnemingen een belangrijke gekoppelde relatie tussen Pex13p afbraak en de import
van matrixeiwitten in peroxisomen. Het is mogelijk dat afbraak van Pex13p de invoer
van matrixeiwitten negatief reguleert door het docking-complex (waarvan Pex13p
onderdeel is) te ontkoppelen van de stroom-afwaartse componenten die nodig zijn voor
de recycling van de PTS1-eiwitimportreceptor Pex5p, zoals het RING E3-complex of de
AAA- ATPasen Pex1p en Pex6p. Aangezien degradatie van Pex13p een snelle en
algemene gebeurtenis is die zich onder verschillende groeiomstandigheden voordoet,
lijkt het echter onwaarschijnlijk dat de afbraak van Pex13p de invoer van matrixeiwitten
negatief regelt. Een andere hypothese is dat degradatie van Pex13p vereist is om het
tijdelijke importomeer-complex te dissociëren. De snelle associatie en dissociatie van
meerdere factoren in het importomeer-complex is waarschijnlijk vereist voor het
importproces en het is mogelijk dat de verwijdering van Pex13p uit het
importomeer-complex het importomeer kan destabiliseren en kan leiden tot de vrijgave
van de eiwitten uit het lumen of het zou kunnen leiden tot de recycling van Pex5p naar
het cytosol. Vandaar dat verder onderzoek vereist is naar de rol van Pex13p-degradatie
bij de invoer van matrixeiwitten.
In Hoofdstuk vier hebben we de afbraak van Pex13p in de S. cerevisiae van gist
onderzocht en een tandem fluorescente eiwit timer (tFT) gebruikt om bijkomende
factoren te identificeren die betrokken zijn bij de degradatie van Pex13p. Onze gegevens
tonen aan dat snelle afbraak van Pex13p geconserveerd is in S. cerevisiae wildtype
cellen die zijn gekweekt op oliezuurmedia, en dat Pex13p wordt afgebroken via UPS.
Dit laat opnieuw zien dat Pex13p turnover waarschijnlijk een belangrijke rol speelt in de
peroxisoombiologie. Bovendien speelt de peroxisomale ubiquitinatie-machine een
belangrijke rol bij de omzet van Pex13p, terwijl de extra cytosolische UPS-factoren
Ufd4p, Ubc4p en Ubr2p een ondergeschikte rol spelen in de Pex13p-turnover, mogelijk
door de vorming van poly-ubiquitine ketens op Pex13p. Het feit dat meerdere E2s en
E3's een rol lijken te spelen bij de afbraak van Pex13p, suggereert dat ofwel
verschillende paden parallel werken op Pex13p, om de afbraak ervan te
vergemakkelijken, ofwel dat al deze factoren samenwerken bij het ubiquitineren van
Pex13p om het eiwit te markeren voor proteasomale afbraak. Bovendien geven deze
waarnemingen aan dat cytosolische UPS-factoren de turnover van PMP's kunnen
reguleren en dus mogelijk invloed kunnen hebben op de peroxisoomfunctie. Dit geeft op
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198
zijn beurt aan dat de afbraak van PMP's, zoals die van ER- en mitochondriale
membraaneiwitten, wordt gereguleerd op het niveau van de algemene cellulaire
eiwitafbraak processen. Tenslotte tonen onze gegevens ook aan dat de functie van
Cdc48p niet vereist is voor afbraak van Pex13p. Aangezien Cdc48p betrokken is bij de
afbraak van ER- en mitochondriale membraaneiwitten, laat deze waarneming zien dat de
afbraak van PMP's anders is dan die van andere membraaneiwitten van organellen, en
laat zien vast dat er verschillende mechanismen bestaan om deze afbraakprocessen
mogelijk te maken. Een mogelijkheid is dat de AAA-ATPasen Pex1p en Pex6p, die
betrokken zijn bij de extractie van ubiquitinated Pex5p van het peroxisomale membraan,
zich richten op ge-ubiquitineerd Pex13p naar het proteasoom. Het membraangebonden
AAA-ATPase Msp1p, waarvan werd gerapporteerd dat het staart verankerde eiwitten uit
het peroxisomale membraan extraheert voor afbraak, kan echter ook worden gezien als
een interessante kandidaat voor verder onderzoek. Ten slotte geven recente rapporten
aan dat het proteasoom kan worden gerekruteerd naar membranen om de afbraak van
membraaneiwitten mogelijk te maken. Misschien bestuurt een dergelijk mechanisme
ook de degradatie van Pex13p. Het is duidelijk dat verder werk nodig is om te
onderzoeken hoe ubiquitinated Pex13p wordt uit het peroxisomale membraan wordt
gehaald.
De peroxisoomfunctie is extreem divers en hangt af van soort, celtype en
groeicondities. Om een volledig begrip van de functie (s) van peroxisomen in een
bepaalde cel onder een gegeven aandoening te hebben, is een volledig overzicht van de
eiwitten in deze peroxisomen van vitaal belang. Op massaspectrometrie gebaseerde
proteomics methoden zijn van onschatbare waarde gebleken bij het bestuderen van het
peroxisomale proteoom en hebben verschillende nieuwe inzichten in de
peroxisoomfunctie verschaft. In Hoofdstuk vijf hebben we de bevindingen samengevat
van verschillende massaspectrometrie-gebaseerde proteomics studies van organellen in
gist en filamenteuze schimmels en hebben we de nieuwe inzichten in de peroxisomale
functie uit de studies geschetst.
PMP's zijn betrokken bij alle peroxisomale functies en zijn daarom van vitaal
belang voor het cel metabolisme. De verdere studie van PMP-afbraak zal ons begrip van
hoe PMP-homeostase in stand wordt gehouden en hoe deze invloed heeft op de
peroxisoomfunctie aanzienlijk verbeteren. In dit proefschrift hebben we de afbraak van
de PMP Pex13p in gist onderzocht en naar de bijdragen gekeken van de ubiquitinatie
machinerie van het peroxisomaal membraan, en andere componenten van de UPS. Het
feit dat Pex13p degradatie ondergaat in twee verschillende organismen, blijkbaar via
soortgelijke mechanismen, suggereert sterk dat het vermogen om Pex13p af te breken
Samenvatting
199
zowel een algemeen kenmerk van peroxisomen is, als ook dat het belangrijk is voor de
functie van Pex13p in het importproces van matrixeiwitten. Als we nog een stap verder
gaan, en aannemen dat degradatie van Pex13p ook in zoogdiercellen voorkomt, kunnen
we ons afvragen hoe degradatie van Pex13p kan bijdragen aan de gezondheid van de
mens en of defecten in de afbraak van Pex13p mogelijk menselijke ziekten kunnen
veroorzaken. Omdat de afbraak van Pex13p in beide organismen de peroxisomale
ubiquitinatie-machinerie vereist, gekoppeld aan eerdere rapporten die een rol laten zien
voor componenten van deze machine in de ubiquitinering en afbraak van extra PMP,
vermoeden we bovendien dat de peroxisomale ubiquitinatie-machinerie in feite een
algemeen ubiquitinatie-platform op het peroxisomale membraan is dat op meerdere
substraten is gericht. Toekomstige studies die gericht zijn op het identificeren van extra
substraten van deze machinerie zullen waardevolle nieuwe inzichten verschaffen in de
rol van de machinerie in de peroxisomale functie.
200
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201
Acknowledgments
Time fleeting, I have witnessed the blossom of trees on campus for five times. Dozens
of people have come to and gone away from the lab in the past few years. I can still
sense the warmth and scent of those memories as if they were happening yesterday. For
a long time, I could not help think that if one day I was no more and then opened eyes to
see this place, the lab, campus and city, and I would perceive myself as entering the
heaven.
My parents do not understand our project, simply not their major, but they supported
me through PhD program with a strong faith and unflinching determination. I would not
be here at the first place without my parents, the source of my life and power.
My first peroxisome meeting OEPM started one week after I joined the lab since Sep,
1st in 2014. Jannet, the Secretary of Molecular Cell Biology and Cell Biochemistry, has
helped me since then with all the paperwork, from the expenses of conferences to my
application of visa. Being skillful, she helped me with patience, politeness and
friendliness, otherwise I would be lost in those files and the plan of project might even
be affected.
The first time I joined lunch with people from the lab, I met several cheerful faces.
Adam and Sanjeev were productive and outgoing, setting a standard for the following
students. Terry was the first Chinese student in the lab. The first day I came to the lab, I
saw him doing Western, putting those bottles as weight onto the lid during the
transferration. Interesting, Western is also the most important assay I have been doing it
for almost four hundred times during my PhD program. Maybe I can consider this as an
inheritage in a way. Ann and Arman were smart and passionate about socializing, always
trying to glue people together with outside lunch at the diner in Bernoulliborgh, or
Christmas party, or summer borrel or drink on the lawn. Natasha, Justyna and Ritika,
like elder sisters, always ready to answer my odds and ends questions frankly. Srishti is
a member of Chris’s group, and she has won several prizes for the best poster in
conferences. The S. cerevisiae work in this thesis was originated from part of her
research, and she helped me a lot with strains and tFT knowledge. I am so glad to have
this team player as colleague in the lab. It was my luck to supervise Joana and Inge for
several months, their intelligence and diligence added colors to the project. For
numerous master and bachelor students, they have contributed and inspired us, bringing
us lively faces and laughter. I still remembered when we sat outside by a big wooden
table for lunch in summer, lively and pleasant.
The first time I joined the seminar, I noticed four men sitting at the back row, Arjen,
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202
Rinse, Kevin and my boss, Chris. I have learned quite a lot from them. Rinse was the
green finger for computers and electron microscopy. Also focused in EM, Kevin was
clever and smelled like grapes. His beard looked like a young version of Santa. Arjen
was friendly, and taught me how to process fluorescence images concisely. When I
walked behind them in Vienna for OEPM in 2016, they seemed like Mr. Bear and Mr.
Giraffe, only in a cute and friendly way. Further thanks to Arjan for keeping the lab
running, and he is important for the group. More thanks to the people from both groups
Molecular Cell Biology and Cell Biochemistry.
My stay here was definitely colorful and warm with these people, but one person far
outshined, Chris. I am still grateful that I was enrolled under his supervision. The first
time I came to the office, he welcomed me with a firm handshake. I still remembered he
showed how to perform Western, PCR and digestion, patient and meticulous. Unlike
others I met in the past who might just threw a protocol to me, Chris showed me each
step carefully and patiently. This made an good and correct opening to my PhD program,
set the right path for the future years. He prepared the computer for me to provide
convenience for my work, printed publications for me to learn background information,
showed me around the instruments and freezers so that I can get familiar with the
chemicals, enzymes and strains. He taught me how to use the database and the protocols,
how to search gene and protein information, and how to design the plasmid construction.
Furthermore, he taught me how to use Photoshop and illustrator to process images, and
how to make plasmid map with CloneManager. He did not just tell which buttons to
click, but carefully taught me about the rationale, the theory and the mechanism, down
to each detail with drawing graphs and figures. I kept each piece of these valuable notes
in my lab journal. He told me that education is not just restricted in college, but lifetime,
and we should not only know “what”, but also actively pursuing the “how” and “why”
with critical thinking.
He is my boss, and a gentleman. Unlike other people I met in the past who maltreated
students, he treated me as a civilized person and talked to me with equal status, respect
and humanity. He talks to me in a man-to-man manner, not a boss to a subordinate, or a
tyrant to a slave, or an elder to a kid, but a man to a man, affable and approachable. If he
needs me to help him with taking out a plate from the incubator, he always gently asked
whether I had time or not, rather than just gave a command. When I helped him with
something, however small it was, he always thanked me. He treated us students equally
with no discrimination or bias, which I really appreciate very much. The way he talks is
sincere and inspiring. He always guided and enlightened me with series of
thought-provoking questions to lead me through and let me realize the key point and
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find the answer. Many a case, I have realized his precise insight and foresight when the
experiment was at a cross. He could always point a direction which later proved to be
correct. That talent and wisdom impressed me, and made me think that the Great Britain
is the original source of modern intelligence.
His enormous effort and serious thought in education is rare and precious. I would
love to revisit the scenes when he showed me how to write a paragraph, how to analyze
an image from the data and how to prepare a poster. He helped me to apply for a talk in
the conference, and helped me with the rehearsal till I could tell a story with our data.
He is always ready to help me. He offered comments and helped me with changes to the
poster and manuscript. He spent a lot of time to refine my chapters in the thesis. If I
could sail through the defense with flying colors, that is all because I have lived in the
sunshine radiated from him. He is our group leader, and he indeed leads us through the
PhD program with his care, wisdom and big hands.
In my last year of PhD program, we suffered from change of wind. Two saints Engel
and Bert opened arms in the mediation and intervention and separated the frenzied tidal
surges to two sides and pointed us a path to overcome obstacles. Two giants Peter and
Marteen stepped forward to offer us help, and guided us with solid contributions. Their
noble morality and seasoned experiences gave us shelter to prevent the attack of huge
waves. Chris has protected us ducklings in the storm and across the war fire with all of
his strengths. We are safe and warm under his wings. Like a flying golden eagle, he
carried us flying over the mountains and across the seas. Working with him and under
his supervision, he is more than a boss, more of a mentor, a friend, a relative, a role
model of father. He is the spiritual leader and morning star we trust and believe in.
Shedding tears, I am gravely sorry for the sacrifice he made only to protect us during
that. Now, we are all well protected, but the eagle has to fly away to another place. We
could never possibly express all of our gratitude, and we will miss you. I would
personally rather to interpret this as a pause rather than an end, hope one day the PMAD
project could be continued, and he can get what he deserves and so much more.
Time flies, and people leave. This made me feel painful and emotional. The past few
years I spent here was not only a period of time, but an organic part of my life, an
essential part of my body. The missing of anyone is a loss to myself. Those faces, those
laughter and those happy moments would keep me accompanied when I am lonely, keep
me warm when I am cold in the future.
I wish I could preserve those memories in a safe and beautiful place in my heart. One
day in the morning, in my dream, I walked towards Linnaeusborgh in sunshine with
magpie flying above, and I would be able to go back to the lab where Arjen waved at me,
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Ritika was making master mix for PCR, Ann was shifting cultures to new medium by
the flame. The radio was on, playing cheerful melody. I checked the Western corner and
solutions I prepared one day before to make sure everything required for Western was in
order. There would be new ideas about projects written on the white board and new
paintings of Chris’s children pasted on the wall. I would walk towards the office and
smell Chris’s scent, and hear the sound of a silver spoon stirring in a porcelain mug,
knowing my boss would have been working by the computer. Then I came to the office
with a slight bow, saying:
“Morning!”
“Morning, Chen!”